Alginases, systems containing alginases and methods of cloning, purifying and/or utilizing alginases

ABSTRACT

The present invention relates to cell wall degradative systems, in particular to systems containing enzymes that bind to and/or depolymerize cellulose. These systems have a number of applications.

CROSS-REFERENCE TO RELATED APPLICATIONS

This claims priority to U.S. Provisional Application No. 60/576,000, filed Jun. 1, 2004, the contents of which are incorporated herein, in their entirety, by reference.

This invention was made with government support under Contract Number SA7528051E awarded by the National Oceanic and Atmospheric Administration and Contract Number DEB 0109869 awarded by the National Science Foundation. The government has certain rights in the invention.

BACKGROUND OF THE INVENTION

1. Field of the Invention

The invention is generally directed to alginases. In particular, the present invention is directed to alginases found in Microbulbifer degradans and systems containing such alginases and methods of cloning, purifying and/or utilizing such alginases.

2. Background of the Invention

Saccharophagus degradans strain 2-40 (herein referred to as “S. degradans 2-40” or “2-40”) is a representative of an emerging group of marine bacteria that degrade complex polysaccharides (CP). S. degradans has been deposited at the American Type Culture Collection and bears accession number ATCC 43961. S. degradans 2-40, formerly known and referred to synonomously herein as Microbulbifer degradans strain 2-40 (“M. degradans 2-40”), is a marine γ-proteobacterium that was isolated from decaying Sparina alterniflora, a salt marsh cord grass in the Chesapeake Bay watershed. Consistent with its isolation from decaying plant matter, S. degradans strain 2-40 is able to degrade many complex polysaccharides, including cellulose, pectin, xylan, and chitin, which are common components of the cell walls of higher plants. S. degradans strain 2-40 is also able to depolymerize algal cell wall components, such as agar, agarose, and laminarin, as well as protein, starch, pullulan, and alginic acid. In addition to degrading this plethora of polymers, S. degradans strain 2-40 can utilize each of the polysaccharides as the sole carbon source. Therefore, S. degradans strain 2-40 is not only an excellent model of microbial degradation of insoluble complex polysaccharides (ICPs) but can also be used as a paradigm for complete metabolism of these ICPs. ICPs are polymerized saccharides that are used for form and structure in animals and plants. They are insoluble in water and therefore are difficult to break down.

Microbulbifer degradans strain 2-40 requires at least 1% sea salts for growth and will tolerate salt concentrations as high as 10%. It is a highly pleomorphic, Gram-negative bacterium that is aerobic, generally rod-shaped, and motile by means of a single polar flagellum. Previous work has determined that 2-40 can degrade at least 10 different carbohydrate polymers (CP), including agar, chitin, alginic acid, carboxymethylcellulose (CMC), β-glucan, laminarin, pectin, pullulan, starch and xylan (Ensor, Stotz et al. 1999). In addition, it has been shown to synthesize a true tyrosinase (Kelley, Coyne et al. 1990). 16S rDNA analysis shows that 2-40 is a member of the gamma-subclass of the phylum Proteobacteria, related to Microbulbifer hydrolyticus (Gonzalez and Weiner 2000) and to Teridinibacter sp., (Distel, Morrill et al. 2002) cellulolytic nitrogen-fixing bacteria that are symbionts of shipworms.

These exo- and extra-cellular structures (ES) include small protuberances, larger bleb-like structures that appear to be released from the cell, fine fimbrae or pili, and a network of fibril-like appendages which may be tubules of some kind. Immunoelectron microscopy has shown that agarases, alginases and/or chitinases are localized in at least some types of 2-40 ES. The surface topology and pattern of immunolocalization of 2-40 enzymes to surface protuberances are very similar to what is seen with cellulolytic members of the genus Clostridium.

2-40 is a gram negative, pleomorphic, motile with a means of a single polar flagellum (see FIG. 1). Cells average 0.5 μm in width and 1.5-3.0 μm in length (Andrykovich and Marx 1988). During late logarithmic-stationary phases of growth, a black pigment, identified as true melanin (Stosz 1994), is produced and cells become elongated (Marx 1986).

The G+C content of 2-40 is 45.66%, as determined by the ATCC (Stosz 1994). 2-40 is catalase- and peroxidase-positive (González and Weiner 2000). It is a strict aerobe capable of respiratory, but not fermentative, metabolism, and requires both sea salts and carbohydrates for growth (Marx 1986, Stosz 1994). It does not form spores or accumulate β-hydroxybutyrate. As an estuarine bacterium, 2-40 is capable of reproduction in a wide range of temperatures (5° C. to 40° C.) and can tolerate 2-10% sea salt. 2-40 can also grow in pH range of 4.5-10, with optimum pH of 7.5 (Gonzalez and Weiner 2000).

2-40 is unique in its capability to degrade numerous insoluble complex polysaccharides (ICP) including alginic acid, agar, cellulose, chitin, glucan, pectin, pullulan, starch and xylan (Whitehead 1997). In addition to its ability to degrade these carbohydrates, 2-40 is also capable of producing lipases, proteases, and tyrosinase (Marx 1986, and Stosz 1994).

Previous studies showed that the cell surface morphology of 2-40 changed when the organism was grown on different insoluble complex polysaccharides (Whitehead 1997). When 2-40 was cultivated on either chitin or agarose, scanning and transmission electron microscopy revealed that the presence of cell surface protuberances, hydrolysomes, correlated to the degradation of these two complex polysaccharides. Other changes in the cell topology and morphology were detected during late growth stages. These changes included production of membranous tubules containing agarases and chitinases. These morphological changes may correlate with the ability of 2-40 to survive dynamic changes in the estuarine ecosystem (Chakravorty 1998 and Whitehead 1997).

Preliminary studies suggested that 2-40 be assigned to genus Alteromonas (Andrykovich and Marx 1988). However, a recent search in the MIDI database revealed that Marinobacterium georgiense is the closest relative to 2-40 based on fatty acid profile. It also revealed a comparatively low level of similarity with that of Microbulbifer hydrolyticus IRE 31, the closest strain to 240 according to its 16S rDNA (Gonzalez and Weiner 2000). Moreover, the GenBank search showed that 2-40 has 93% similarity with Microbulbifer hydrolyticus, and 91.2% similarity with a cellulytic nitrogen-fixing bacterium, isolated from the gland of Deshayes in three different species of shipworm (González and Weiner 2000). While the taxonomy is not yet fully settled, based upon the 16S rDNA analysis, strain 2-40 was placed in genus Microbulbifer as a new species, Microbulbifer degradans. It is a member of the γ-subclass of the phylum Proteobacteria (González and Weiner 2000 and Weiner et al., 2000).

Marsh grass Spartina alterniflora is found to be the most common species in the salt marshes of the east coast of North America (Ford 1993). In addition to S. alterniflora, which is a dominant species at mid level of elevations, Spartina patens and Distichlis spicata dominate at high elevation while Zostera marina and brown algae are common in low marsh elevation (Chakravorty 1998). Salt marsh grass supports a wide range of algal population, including green, brown, blue-green, and red algae, in addition to a diverse bacterial, fungal, protozoan, and invertebrate populations (Stosz 1994). 2-40 was shown to have capabilities to produce different degradative enzyme systems and to utilize a variety of substrates, all of which increase the organism's ability to survive in this environment. It can also naturally recycle several ICPs, thus may be employed in bioremediation (Chakravorty 1998).

In natural environments, numerous amounts and various kinds of ICPs are formed and accumulate leading to the requirement for efficient mechanisms for their degradation. As part of the carbon cycle, they are recycled to their primary elements (Whitehead 1997 and Chakravorty 1998). These ICP, composed of homo- and heteropolysaccharides, account for substantial agriculture, aquaculture and algalculture wastes. With the exception of starch, these compounds compose the cell wall structure in plants and fungi (Whitehead 1997). Because of their binding, branching sugar composition, and complexed formation with other polymers, the degradation of ICPs is not a trivial process. However, these ICPs can be hydrolyzed by microorganisms to produce monosaccharide feedstock. For example, in the marine environment, around 10¹¹ tons of chitin wastes are produced annually, yet, apart from living or recently living biota, only traces of it are found in marine sediments. This is explained by the presence of microorganisms that degrade chitin and recycle the carbon and nitrogen (Salyers et al., 1996). For economical and environmental considerations, biomerediation, using prokaryotes is an efficient way to recycle ICP. Bacteria and fungi degrade ICP to provide saccharide feedstock (Salyers et al., 1996).

In addition to feedstock, degradation of alginic acid yields 4-deoxy-L-erythro-hex-4-ene-pyranosylurinate containing oligosaccharides, which are thought to be active biological molecules. These oligosaccharides can elicit plant germination, shoot elongation and root growth promoting activities (Natsume et al., 1994). They also stimulate the growth of Bifidobacteria, a useful food industry organism (Akiyama et al., 1992).

Alginic acid is a high molecular weight linear polysaccharide polymer produced mainly by seaweed, as well as many species of marine algae and certain bacteria (Linhardt et al., 1986 and Chakravorty 1998). It is comprised of (1-4)-linked β-D-mannuronic acid (M) and α-L-guluronic acid (G), (See FIG. 2), (Gacesa 1992). The salts of alginic acid are commonly referred to as alginate, which include: ammonium alginate, calcium alginate, potassium alginate, and sodium alginate (Chakravorty 1998). The primary structure of alginic acid is highly variable based on the monomer ratios and distribution of monomers into homopolymeric blocks (GG or MM) or heteropolymeric blocks (MG) (Doubet and Quatrano 1982).

The composition of alginate greatly depends on the producing organism and its physiology. Algal alginates are unbranched (1-4) linked glycuronans containing residues of β-D-mannosyluronic acid and the C5 epimer α-L-gulosyluronic acid, whereas bacteria normally produce their alginate being invariably O-acetylated, where O-acetyl groups are found on the 2 and/or 3 positions of D-mannuronate residues (Gacesa 1988). This acetylation often affects water-binding properties and ion-binding selectivity of the polymer (Wong et al., 2000). The level of alginate's susceptibility to degradation is normally influenced by both the block structure and degree of O-acetylation within the macromolecule (Wong et al., 2000).

Algal and bacterial alginates also differ in their molecular weight. Alginate produced by A. vinelandii has a molecular weight of 2×10⁶ Da, whereas algal alginates have a range of 48000 to 186000 Da; in general, bacterial alginates usually have higher molecular mass than algal polymer (Pe{umlaut over (n)}a et al., 2002).

Alginate, a viscous polysaccharide, is found in the cell wall of the brown seaweeds (Phaeophyceae) and produced by several species of bacteria. Like its structure, the function of alginate varies depending on its source. In brown algae, alginate comprises about 60% of the cell wall mass of Fucus distichus (Doubet and Quatrano 1982). Approximately 22,000 tons/annum of alginate are extracted from numerous brown algal genera to be used in a variety of applications by the food, pharmaceutical and other industries. Most of the commercial alginate is extracted mainly from genera Macrocystis, Laminaria, and Ascophyllum (Wong et al., 2000). The brown algae alginate is believed to function as an intercellular skeletal matrix (Ertesvåg et al., 1995).

In addition to the brown algae, alginate is also produced by two bacterial families, Azotobacteriaceae and Pseudomodacease (Wong et al., 2000). Azotobacter vinelandii, A. chroococcum, Pseudomonas aeruginosa and other Pseudomonads synthesize alginate as an extracellular polysaccharide (Gacesa 1992), and as a major component of many biofilms (Weiner et al., 1998). It has its ability to form viscous solutions at relatively low concentrations and to form gels with Ca⁺² (Davidson et al., 1976).

Alginate is enzymatically degraded by a group of enzymes that catalyze the β-elimination of the 4-O— linked glycosidic bond forming unsaturated uronic acid-containing oligosaccharides (Preiss and Ashwell 1962a, Kiss 1974, Caswell et al., 1986, Gacesa 1992, and Wong et al., 2000).

Alginases, typically lyases, are members of the class polysaccharide lyases, or eliminases, (EC 4.2.2.-). They normally act in a wide range of naturally acidic polysaccharides. Enzymes of this class have low or intermediate molecular weight (20-110 kDa) and are characteristically, usually, monomeric, having the same molecular weight when determined under reducing or non-reducing conditions. They act through a β-elimination mechanism (Haugen et al., 1990), rather than hydrolysis, to cleave certain glycosidic linkage in the acidic polysaccharides. This reaction results in unsaturated oligosaccharide products (uronic acid residues) at the new non-reducing end (Haugen et al., 1990, Linhardt et al., 1986). Polysaccharides cleaved by elimination generally contain a carboxylate group on the carbon adjacent to the glycosidic linkage (Haugen et al., 1990, Gacesa 1992). However, one group reported that alginases are hydrolyases (Schaumann and Weide, 1990), where the enzyme was isolated from marine fungi, Dendryphiella salina and Asteromyces cruciatus. The mechanism of action of this enzyme, though, is not fully understood (Gacesa 1992).

Alginate lyase (EC 4.2.2.3) catalyzes the reaction of alginate degradation by elimination mechanism (Romeo and Preston 1986b, Linhardt et al, 1986, Gacesa 1992, Wong et al., 2000). This reaction targets the glycosidic 1→4 O-linkage between alginate monomers. The results are: a) formation of double bond between the C4 and C5 of the six-carbon ring, from which the 4-O-glycosidic bond is eliminated; b) depolymerization of alginate; and finally c) a product containing 4-deoxy-L-erythro-hex-4-enopyranosyluronic acid as the non-reducing terminal (Gacesa 1992 and Wong et al., 2000).

Alginases are normally utilized to degrade alginate as a carbon source; however, interestingly alginate-producing organisms are not usually capable of growing on alginate as the sole source of carbon. On the other hand, organisms capable of utilizing alginic acid as a sole source of carbon produce both exo- and endolytic alginases, unless they exhibit commensalisms with another organisms to degrade the complex polysaccharide to monomeric subunits (Gacesa 1992).

Alginate lyases have been isolated from different organisms including marine algae, marine bacteria, marine mollusk, fungi, and a wide variety of microorganisms (Hansen et al., 1984, Gacesa 1992, Wong et al., 2000).

TABLE 1.1 Alginase producing organisms. Organism Source Enzyme Reference 2-40 (Microbulbifur salt marsh grass alginic acid lyase Marx 1986, Stosz 1994, degradans) bacterial isolates Whitehead 1997, this study Agrobacterium tumefaciens Genome alginic acid lyase Goodne et al., 2001 str. C58 sequence¹ Alginovibrio aqualiticus marine bacterium alginic acid lyase Stevens & Levin 1977 Alteromonas sr. strain KLIA marine bacterium alginic acid lyase Sawabe et al., 1997 Alteromonas spp. soil bacterium alginic acid lyase Vilter 1986 Aplysia spp. Mollusks alginic acid lyase Kloareg et al., 1989 Asteromyces cruciatus marine bacterium alginic acid Schaumann & Weide hydrolyase 1990 Azotobacter chroococcum soil bacterium alginic acid lyase Kennedy et al., 1992 Azotobacter vinelandii soil bacterium alginic acid lyase Kennedy et al., 1992 Bacillus circulans soil bacterium alginic acid lyase Hansen et al., 1984 Bacillus halodurans Genome alginic acid lyase Takami et al., 1999 sequence¹ Bacteriophage that infects Phage alginic acid lyase Davidson et al., 1977 A. vinelandii Beneckea pelagia marine bacterium alginic acid lyase Pitt & Raisbeck 1978 Chlorella virus virus alginic acid lyase Suda et al., 1999 Choromylitis meridonalis Mollusk alginic acid lyase Seiderer et al., 1982 Clostridium grantii soil bacterium alginic acid lyase Mountfort et al., 1994 Corynebacterium spp. soil/marine alginic acid lyase Matsubara et al., 1998 bacterium Dollabella auricular Mollusk alginic acid lyase Nishizawa et al., 1968 Enterobacter cloacae soil/marine alginic acid lyase Shimokawa et al., 1997 bacterium Fucus zygotes brown algae alginic acid lyase Vreeland & Laetsch 1990 Haliotis corrugate Mollusk alginic acid lyase Linhardt et al., 1986 Haliotis rufescens Mollusk alginic acid lyase Linhardt et al., 1986 Haliotis tuberculata Mollusk alginic acid lyase Kloareg & Quatrano 1987 Katherina tunicate Mollusk alginic acid lyase Kloareg & Quattrano 1987 Klebsiella pneumoniae soil/marine alginic acid lyase Boyd &Turvey 1977, bacterium Lange et al., 1989 Laminaria digitata brown algae alginic acid lyase Madgwick et al., 1978 Littorina spp. brown algae alginic acid lyase Elaykova & Favorov 1974 Mesorhizobium loti Genome alginic acid lyase Kaneko et al., 2000 sequence¹ Pelvetia canalitulata brown algae alginic acid lyase Madgwick et al., 1978 Perna perna Mollusk alginic acid lyase Seiderer et al., 1982 Photobacterium spp. marine bacterium alginic acid lyase Romeo & Preston 1986a Pseudoalteromonas alginic acid lyase Sawabe et al., 2001 elyakovii Pseudomonas alginovora marine bacterium alginic acid lyase Chavagnat et al., 1996 Pseudomonas aeruginosa marine bacterium alginic acid lyase Linker et al., 1984 Pseudomonas maltophilia marine bacterium alginic acid lyase Sutherland & Keen 1981 Pseudomonas putida marine bacterium alginic acid lyase Conti et al., 1994 Pseudomonas syringae pv. Plant pathogen alginic acid lyase Ott et al., 2001 phaseolicola Pseudomonas syringae pv. Plant pathogen alginic acid lyase Preston et a., 2000 syringae Salmonella enterica subsp. Genome alginic acid lyase Parkhill et al., 2001 enterica serovar typhi sequence¹ Sphingomonas species Al alginic acid lyase Yoon et al., 2000 Spinula solidissima Mollusk alginic acid lyase Jacober et al., 1980 Staphylococcus aureus Genome alginic acid lyase Baba, et al., 2002 subsp. aureus MW2 sequence¹ Turbo corrutus Mollusk alginic acid lyase Muramatsu et al., 1977 Undaria pinnatifida brown algae alginic acid lyase Watanabe & Nishizawa 1982 Vibrio alginolyticus marine bacterium alginic acid lyase Kitamikado et al., 1992 Vibrio harveyi marine bacterium alginic acid lyase Kitamikado et al., 1992 Xanthomonas axonopodis Genome alginic acid lyase Da Silva et al., 2002 pv. citri str. 306 sequence¹ Yersinia pestis KIM Genome alginic acid lyase Deng, et al., 2002 sequence¹ ¹Genome sequence obtained from National Center for Biotechnology Information (NCBI) data base, (www.ncbi.nlm.nih.gov). Table partially adapted from Chakravorty 1998.

Table 1.2 illustrates alginase properties from some marine and other gram-negative bacteria. The table shows that optimum pH for most alginases ranges around neutral; specifically it falls in between 6-8.5, while optimum temperature for alginases from different sources has a broad range.

Alginate monomers are linked by 4-O-glycosidic bonds. These bonds can be chemically degraded either by lyase activity (Haug et al., 1967, Doubet and Quatrano 1982) or reportedly by alkali-catalyzed β-elimination (Kiss 1974). The alkali may actually disrupt all polysaccharide linkages being non specific for alginate linkages.

Alginase, and well as other degradative enzymes produced by 2-40 could be useful bioremediation tools. As human population increases and more food is required, agricultural, aquacultural, and algalcultural wastes also increase and can become a serious problem. The wastes are mostly recalcitrant complex carbohydrates, namely cellulose, chitin and agar. The complex carbohydrates from natural and human practices are composed of monosaccharide, many of which can provide valuable feedstock when hydrolyzed. The degradative protuberances of 2-40 could be used as bioremediation tools when used as concentrated, organized, protective enzyme packets.

TABLE 1.2 Alginate lyases from marine and gram-negative bacteria: localization and properties. Molecular Endo/ weight Opt Source Localization^(a) Exolytic (kDa) pl pH Opt T Ref. Marine bacteria Alginovibrio aquatilis Extracellular Endolytic 110 — 8 — Stevens and Levin 1977. Alteromonas sp. Extracellular Endolytic 32 4.7 7.5 30 Sawabe et al., Strain H-4 1992, Sawabe et al., 1997. Beneckae pelagia Intracellular — — — 8 25 Sutherland and Keen 1981 Extracellular — Pitt and Raisbeck 1978 Halomonas marina Intracellular — 39 7.78 — — Kraiwattanapon et al., 1999 Photobacterium sp Periplasm (R) Endolytic 30 6 — — Malissard et al., (ATCC 433367) 1995. Malissard et al., 1993. Pseudomonas sp. Intracellular/ Endolytic 94 — 7.5 — Muramatsu and (marine) Extracellular 32 — 7.5 — Sogi, 1990 Pseudomonas Extracellular Endolytic 32 5.5 7.5 — Boyen et al., 1990 alginovora (strain X017) Vibrio sp. (marine Extracellular — — — 8.5 45 Chavagnat F, et bacterium) al. 1996. Takeshita and Muramatsu 1995 Takeshita et al., 1993 Vibrio alginolyticus Extracellular Endolytic 47 4.6 8.2 — Kitamikado et al., ATCC 17749 1992, Kitamikado et al., 1990. Vibrio halioticoli NA NA 252aa NA NA NA Wong et al., 2000. Vibrio harveyi AL-128 Extracellular Endolytic 57 4.3 7.8 — Kitamikado 1992, Kitamikado et al., 1990, Tseng et al., 1992 Gram-negative bacterial A. chroococcum Periplasm Endolytic 43 — — 30 Peciña and Paneque 1994, Peciña et al., 1999 A. vinelandii Intracellular — ~50 — 7.5 — Davidson et al., 1977 Enterobacter cloacae Extracellular Endolytic 32-38 8.9 7.8 30 Nibu et al., 1995 M-1 pl: isoelectric point, the pH at which a molecule carriers no net electric charge. Opt pH: optimum pH, Opt T: Optimum temperature.

TABLE 1.2 Alginate lyases from marine and gram-negative bacteria: localization and properties (cont'd). Molecular Endo/ weight Opt Source Localization^(a) Exolytic (kDa) pl pH Opt T Ref. K. aerogenes type Intracellular Endolytic 28-31.6 — 7 37 Lange et al., 1989. 25 Extracellular Endolytic — — 7 — Boyd and Turvey 1977, Haugen et al., 1990 K. pneumoniae Extra/intracellular — 28 8.9 — — Caswell et al., 1989 subsp. aerogenes (R) P. syringae pv. Periplasmic Endolytic 40 8.2 7 42 Wong et al., 2000 syringae Pseudomonas sp. Intracellular — 90, 72, — — — Kraiwattanapong et OS-ALG-9 60, 54 al., 1997 Sphingomonas sp. Cytoplasm Endolytic 60  9.03 7.5-8.5 70 Yonemoto et al., 1991, Yonemoto et al., 1993, Yonemoto et al., 1992. Streptomyces NA NA 259aa NA NA NA Redenbach et al., coelicolor 1996 —: Not determined, NA: not available, ^(a)Localization in native culture, except R, R = recombinant expression in E. coli. N/A: not available, Opt: optimum, T: temperature ° C., aa: amino acid residues. Adapted from Wong et al., 2000.

Alginase has potential medical importance. The alginate glycocalyx abundantly produced by mucoid strains of Pseudomonas aeruginosa is considered a major virulence factor in endocarditis (Bayer et. al., 1992). It also contributes to the morbidity and mortality associated with pseudomonal infections in patients with cystic fibrosis (Dinwiddie 1990, Gacesa, P. 1988) where alginate promotes attachment to the host cell and inhibits the phagocytosis (Bayer et al., 1992, Gacesa 1992, Monday and Schiller 1996).

Pseudomonas aeruginosa is one of the most important opportunistic human pathogens, causing septicemia and severe or even lethal infection to the respiratory tract, urinary tract, intestines and many other sites (Cross et al., 1983). This organism exhibits inherent resistance to a wide range of antibiotics, which makes infection with this pathogen common and hard to treat (Monday and Schiller 1996).

In a recent study, the effect of alginase on the polymorphonuclear leukocyte (PMN)-directed and antibiotic-mediated phagocytosis and killing of mucoid P. aeruginosa was investigated both in vitro and in vivo. The study showed that pretreating of mucoid P. aeruginosa strain 144MR with alginase significantly enhanced PMN phagocytosis, rendering the bacteria more susceptible to PMN-mediated killing than 144MR cells not treated with alginase (P<0.05), approximating the levels of that of non-mucoid strain, 144NM. More importantly, the study also showed that treating the mucoid strain 144MR with alginase caused a significant removal of bacterial cell surface alginate as determined by immunofluroscence staining with a murine monoclonal anti-alginate antibody (Bayer et. al., 1992).

SUMMARY OF THE INVENTION

One aspect of the present invention is directed to systems of alginases and related proteins.

A further aspect of the invention is directed to a method for the degradation of substances comprising alginate. The method involves contacting the alginate containing substances with one or more compounds obtained from Saccharophagus degradans strain 2-40.

Another aspect of the present invention is directed to groups of enzymes that catalyze reactions involving alginate.

Another aspect of the present invention is directed to polynucleotides that encode alginase polypeptides.

A further aspect of the invention is directed to chimeric genes and vectors comprising genes that encode alginase polypeptides.

A further aspect of the invention is directed to a method for the identification of a nucleotide sequence encoding an alginase polypeptide from S. degradans. An S. degradans genomic library can be constructed in E. coli and screened for the desired activity. Transformed E. coli cells with specific activity are created and isolated.

Further aspects of the invention are directed to utilization of the alginase substances in food, beer, wine, animal feeds, textile production and laundering, pulp and paper industry, agricultural and other industries.

Other aspects, features, and advantages of the invention will become apparent from the following detailed description, which when taken in conjunction with the accompanying figures, which are part of this disclosure, and which illustrate by way of example the principles of this invention.

BRIEF DESCRIPTION OF THE FIGURES

FIG. 1 shows a transmission electron micrograph of 2-40 strain;

FIG. 2 illustrates the structure of alginic acid;

FIG. 3 shows alginase activities as a function of time;

FIG. 4 shows thermostability of alginase;

FIG. 5 shows alginase shelf-life;

FIG. 6 is a plot of alginase activity rate as a function of alginic acid concentration;

FIG. 7 is a plot of alginase initial velocity as a function of the reciprocal of the alginate concentration;

FIG. 8 shows domain structure of the S. degradans 2-40 alginases;

FIGS. 9 a and 9 b show an alignment of alginase proteins(9A: SEQ ID NOS 1-7; 9B: SEQ ID NOS 8-10);

FIG. 10 are plots of the growth and alginase production of S. degradans 2-40 as functions of carbon source in the growth medium;

FIGS. 11 and 11 a are plots of the growth and alginase production of S. degradans 2-40 as functions of alginate, glucose, or xylose as the main carbon source in the growth medium.

FIG. 12 are plots of the growth and alginase production of S. degradans 2-40 as functions of alginate concentration in the minimum medium;

FIG. 13 are plots of S. degradans 2-40 alginase production as a function of growth factors requirement;

FIG. 14 are plots of the growth and alginase production of S. degradans 2-40 as a function of concentration of sea salt;

FIGS. 15 and 15 a are plots of the growth and alginase production in combinations of alginate and glucose;

FIG. 16 are plots of the scale-up production of alginase by S. degradans 2-40;

FIG. 17 shows separation of S. degradans 2-40 alginases and a zymogram gel;

FIG. 18 shows electrophoresis of S. degradans 2-40 alginase and a zymogram gel;

FIG. 19 shows separation of S. degradans 2-40 alginases and a zymogram gel;

FIG. 20 shows alginase activities as a function of incubation temperature;

FIG. 21 shows a predicted pathway for alginic acid degradation and transport;

FIG. 22 shows the alginate backbone structure;

FIG. 23 shows the backbone structure of calcium poly-a-L-guluronate left-handed helix;

FIG. 24 shows a plot of alginase production as a function of alginate concentration;

FIGS. 25 a-c are plots of alginase production as a function of casein concentration, peptone concentration and yeast extract, respectively;

FIG. 26 is a plot of alginase production as a function of carbon source;

FIG. 27 is a plot of alginase production as a function of Instant Ocean concentration; and

FIGS. 28 (a and b) and 28 b are plots of related to shake flask and fermenter cultures.

DETAILED DESCRIPTION

Analysis of the genome sequence of S. degradans 2-40 reveals an abundance of genes coding for enzymes that are predicted to degrade plant-derived carbohydrates. To date, 2-40 is the only sequenced marine bacterium with apparently complete cellulase and xylanase systems, as well as a number of other systems containing plant-wall active carbohydrases.

In addition to cellulase, mannase, agarase, pectate lyases, arabinosidase, β-galacosidase, chitinase, and endogluconase, eleven alginate lyases were identified. Alginase genes were determined using [tblastn]¹, in which protein query sequences of alginases of other sources were compared against 2-40 nucleotide genomic sequence, which has been translated in all six reading frames. Protein sequences of alginases from other microorganisms were obtained from the National Center for Biotechnology Information (NCBI) database.² ¹ tblastn compares the protein “Sequence 1” against the nucleotide “Sequence 2” which has been translated in all six readings frames.² Established in 1988 as a national resource for molecular biology information, NCBI creates public databases, conducts research in computational biology, develops software tools for analyzing genome data, and disseminates biomedical information.

Gene models were figured using three gene modeling programs on the all contigs. These programs were: (1) Generation (ORNL)³ uses predominantly 6-mer statistics to recognize coding regions; it uses a proximity rule-based start call with ATG and GTG as potential starts. (2) Glimmer uses interpolated Markov models (IMMs) to identify the coding regions; it uses ATG, GTG, and TTG as potential starts. (3) Critica (v1.05) uses blastn to produce alignments from the entire dataset and derives dicodon statistics to recognize coding sequences. It uses ATG, GTG, and TTG as potential starts. The Generation and Glimmer training set selected consisted of non-overlapping open reading frames (ORFs) greater than 900 bp in length, Doe Joint Genome Institute.]³ Oak Ridge National Laboratory: conducts genetics research and system development in genomic sequencing.

A number of bacteria and fungi synthesize alginases. However, 2-40 is prodigiously degrading alginic acid, and therefore deemed a promising vehicle for producing alginate degrading enzymes. Additionally, since 2-40 also synthesizes at least 10 additional carbohydrase systems, alginase production could serve a paradigm for the efficient production of other degradative enzyme systems.

Improving and increasing the efficiency of microbial digestion, i.e. bioremediation, of alginate, for the present study, and cellulose, chitin, and other biomass of complex polysaccharides, in general, could not only result in reducing the accumulation of wastes, but could also help in production of alternative feedstock, fuels and/or chemicals. For this reason, 2-40 may be exploited for bioremediation of multiple complex polysaccharides, in general, and of alginate in specific that are environmentally and medically important.

So far, few alginases are commercially available. Alginases that can be employed clinically, in turning kelp harvest waste into feedstock, and in bioremediating indigenous biofilms are still required (Weiner et al., 1998). Purification of more effective and readily available alginase would be of great significance in both of these applications.

Alginases from marine bacterium, 2-40, can be produced, concentrated and purified in large quantities to potentially bioremediate alginic acid-containing biofilm.

The genome sequence of 2-40 was recently obtained in conjunction with the Department of Energy's Joint Genome Initiative (JGI). The finished draft sequence dated Jan. 19, 2005 comprises 5.1 Mbp contained in a single contiguous sequence. Automated annotation of open reading frames (ORFs) was performed by the computational genomics division of the Oak Ridge National Laboratory (ORNL), and the annotated sequence is available on the World Wide Web

Experimental Approach: Previous studies showed that 2-40 degradative systems were induced by the corresponding homologous carbon source (Stosz 1994 and Whitehead 1997). 2-40 alginase was repressed by glucose and maximally induced by alginic acid and xylose (Whitehead 1997).

In order to maximize the yield of alginases, the composition of the growth medium was modified from the minimal medium used in the previous work on 2-40 (Chakravorty 1998). Unless otherwise noted, in the following experiments all concentrations are weight/volume. For the following experiments, 2-40 inocula were always exponentially grown at 25° C. in minimal medium (Table 2.1), supplemented with 0.2% glucose, pH 7.6 to a concentration of 10⁴ cells/ml.

The initial experiments were batch fermentations carried out in 250 ml Erlenmeyer flasks, agitated at 200 rpm with rotary shaker, and incubated at 25° C. During the course of growth 2-40, cell number was determined by Total Viable Count (TVC). Alginase activity was assayed in the spent media (supernatant) fractions by DNSA (3,5-Dinitrosalicylic acid) standard procedures, described later. The chemicals and buffers, with their cost, are listed in Table 2.2.

Growth conditions were optimized to increase the enzyme yield. 2-40 was grown in minimal media containing a final concentration (wt/v) of 0.2% of one of 7 different carbon sources, alginate, fructose, glucose, sorbitol, xylose (Sigma), galactose (Fisher), and lactose (Difco), Table 2.1. Cultures were incubated at 25° C., in 250 ml baffled flasks filled with 100 ml of medium, with agitation at 200 rpm on a rotary shaker for 32 hr. This generally corresponded to the start of the decline phase. Every four hours, a sample was withdrawn to assess growth and alginase activity (Procedure details described later).

TABLE 2.1 Composition of Minimal Growth Media Concen- Cost Name Composition tration Source (USD) Minimal Instant Ocean 2.3% Aquarium $2.5/kg medium (sea salts) Systems, France Yeast Extract 0.1% Difco, US $185/kg (YE) Polysaccharide 0.2% (see text) See table 3.1a, p. 52 1M Tris-HCL, 50 mM Sigma, $82/kg pH 7.6^(a) USA NH₄Cl 0.05% Fisher $42/kg Scientific, USA Plate Minimal $0.75/Liter medium medium + 1.5% agar^(b) ^(a)Tris-HCl and NH₄Cl were separately filter-sterilized then added after autoclaving and sufficient cooling since Tris-HCl acts a nitrogen-chelating factor at high temperature, making nitrogen unavailable for the organism growth. ^(b)Plate media did not require the addition of polysaccharide, since 2-40 is capable of utilizing agar as the sole carbon source Cost: all are costs are calculated in US dollars.

TABLE 2.2 Chemicals, buffers, and reagents^(a) Name of chemical, Cost buffer, or reagent Description Source (USD) Alginic acid Sodium Salt, from Sigma $126/kg Macrocystis pyrifera (Kelp) Casein Enzymatic digest of Gibco $115/kg hydrolysate casein laboratories DNSA 3,5-Dinitrosalicylic Sigma $212/kg acid DNSA reagent 0.63% DNSA, 2.14% Prepared ND NaOH, 0.5% phenol in the lab Native-PAGE 10x Tris/Glycine BIO-RAD ND Tank buffer Buffer, pH 8.3 Native-PAGE 0.125 M Tris, pH 6.8, Prepared ND sample 20% glycerol, 0.1% in the lab loading buffer brome phenol blue Peptone Bacto-Peptone Difco $37/kg PIPES buffer 20 mM, pH 6.8 Sigma ND (adjusted with NaOH) SDS-PAGE Tank 0.1% SDS added to BIO-RAD ND buffer native buffer SDS-PAGE native-PAGE loading Prepared in the ND sample buffer + 4% SDS lab loading buffer ^(a)listed alphabetically Cost: all costs are calculated in US dollars. ND: determined.

Results of the initial experiment confirmed that alginic acid induced the highest 2-40 alginase productivity (see Results section for detailed description), hence, it was expected that when the inducer's concentration, i.e. alginic acid, increases, the yield of alginase, in turn, would also increase. This was shown by using minimal growth medium supplemented with alginic acid (Sodium salt from Macrocystis pyrifera [Kelp] Sigma) at various concentrations (wt/v), ranging from 0.1 to 0.6% for 48 hrs n order, to obtain the highest enzyme yield. All cultures were incubated at 25° C., pH 7.6. Samples were withdrawn every 4 hrs to monitor biomass growth and measure the alginase activity.

Previous work has shown that yeast extract was stimulatory for growth and/or alginase synthesis. To determine the requirements of 2-40 for vitamins and/or amino acids for alginase synthesis, minimal medium, with (wt/v) 0.5% alginate and 2.3% IO,was supplemented with either yeast extract (YE), casein hydrolysate (C), as a rich source of amino acids, or peptone (P) at a range of concentrations between 0.0 and 2.0%. These media were inoculated with 2-40 which was cultures as described above.

Marine bacterium 2-40 requires sea salt. Thus, the effect of the sea salt (Instant Ocean) concentration on growth and alginase production of 2-40 was investigated by the following procedure: 0.5% alginate/0.2% YE (wt/v) minimal medium was supplemented with different concentrations of Instant Ocean (IO): 1, 2.3, 3.5, 5, and 7% (wt/v) inoculated with 10⁴ cells/ml 2-40 inoculum and at 25° C., agitated by rotary shaker at 200 rpm and grown for 48 hrs. Samples were withdrawn every 4 hrs to monitor growth and alginase activity.

When present in growth media, glucose supported a high yield of biomass, at the same time it repressed alginase activity. To increase biomass, glucose, at different concentrations (wt/v) ranging from 0.0 to 0.2%, was included with alginate minimal medium in concentration (wt/v) from 0.5 to 0.3%, to make the final concentration (wt/v) of carbon 0.5%. The purpose of this strategy was to build biomass as 2-40 used glucose and then turn on enzyme activity as the glucose was consumed and 2-40 switch to alginate. During the incubation time period, growth was determined, and both alginase activity and glucose consumption were measured.

In preliminary experiments, it was found that a medium composed of 0.05% glucose, 0.45% alginate, 3.5% sea salts, and 0.2% Yeast extract (wt/v), (pH 7.6) enhanced alginase productions compared with similar semi-defined medium without glucose. To confirm these results, 2-40 was grown in a 250 ml Erlenmeyer flask containing 100 ml of the alginase production medium (APM), described above, for 48 hrs at 25° C. with 200 rpm shaking speed. Throughout the incubation time, growth was determined using OD change and alginase activity was assayed using the DNSA procedure.

2-40 was grown in a 14-L stirred fermentor (Microferm Fermentor, New Brunswick Scientific, N.J.) filled with 8L of the APM, that was used in the flask experiment. The conditions used were 25° C., agitation at 400 rpm, aeration at 6000 cc/min, no pH control and a 2% 2-40 inoculum. Under these conditions, the organism was grown for 52 hrs. During the incubation period, samples were withdrawn to monitor growth calorimetrically and to detect alginase activity by the DNSA method.

To prevent excessive foam build-up, oil-based antifoam was added to the fermentor medium prior autoclaving. In fermentation, the fermentor reactor can be divided into two zones, the first is liquid zone where fermentation processes happen and diffused air occurs as bubbles and as an oxygen source. The second zone is the foam phases which is relatively inert, has a high volume portion of air and contain a large amount of long-living lamellae, the thin film separating two bubbles. Formation of foam takes two stages; (1) drainage, which is water flow from the foam phase, driven by gravity and curvature, and (2) bubble rupture which occurs when the lamellae, separating two bubbles, rupture. The antifoam mechanism works by enhancing the rate of lamellae rupture. First, emulsion droplets collide with air bubbles resulting in the deposition of the antifoam particles onto the air bubble surfaces, followed by the deform of emulsion droplets to produce lenses on the water/air interface (Pelton 2002).

Data of alginase activity of the above fermentation experiments were statistically analyzed by a linear model (Glantz 2002) using the SAS system program for Windows, version 8, 1999.

Total Viable and Biomass Count. At each time point, samples were taken and the total viable count and optical densities (600 nm) were determined in triplicate. For total viable counts, minimal media agar plates were used. In this case agar was the sole source of carbon. The Ultroscopec 2000 (Pharmacia Biotech) was used for all photometric measurements (Optical density). Determination of alginase activity by DNSA reducing sugar assay. This method was developed by Sumner and Sisler (Sumner and Sisler. 1944). At each time point, one ml culture sample was centrifuged at 10,000×g/10 min at 4° C. (using Biofuge A centrifuge, American Scientific Products) and the supernatant was stored at −20° C. until assayed. In this procedure, 0.3 ml of the supernatant fraction or enzyme preparation was incubated with 0.7 ml of substrate (0.5% sodium alginate in phosphate buffer, pH 7.0) for 30 min at 25° C. After incubation, 1 ml of DNSA (Dinitrosalicyclic acid) reagent (2.14% NaOH, 0.63% DNSA, 0.5% phenol) was added to the reaction mixture and samples were boiled for 5 min., cooled under tap water and measured for absorbency at 575 nm. Buffer was used as blank. Negative control contained 0.3 ml sterile medium and 0.7 ml buffer. The amount of reduced sugar produced by the reaction was determined by comparing each OD measurement to a linear regression (100 to 500 μg/ml) of galactose concentrations. For each new preparation of DNSA reagent, a galactose standard curve was plotted. One unit of alginase enzyme was defined as the amount of enzyme that produces 1.0 μg of reducing sugar (measured as D-galactose) from alginic acid per 30 min at pH 7.0 and 25° C. Proteins concentration (BCA Assay). The protein content of each sample was determined according to PIERCE BCA protein Assay (Pierce Rockford, Ill.) as outlined by the manufacturer. The BCA assay is a sensitive, stable and highly specific reagent. In this reaction, protein reacts with Cu²⁺ in an alkaline medium, producing Cu¹⁺. A detectable purple color product, formed by the reaction of two molecules of BCA with one cuprous ion (Cu¹⁺), is measured at 540 nm.

Procedurally, 10 μl of the enzyme preparation (supernatant fraction) was incubated with 200 μl of working reagent (composed of 1:50 dilution of reagent A:B) for 30 min at 37° C. in 96-well ELISA plate. The color was then measured at 540 nm. For calculating the protein concentration, a standard curve was constructed using a serial dilution of 20 to 200 □g/ml of Bovine serum albumin (BSA) with each newly prepared batch of BCA reagent.

In order to obtain the maximum yield of alginase, 8 L of optimized growth medium, defined by the results of the previous experiments, were inoculated with 24 hr 2-40 culture. Culture was incubated for 32 hr, where alginase production reaches its peak. At the end of the incubation period (32 hr), alginase was separated from cells by centrifuging the culture at 10000×g for 20 min/4° C. Cells were harvested and the cell-free supernatant, containing alginase, were concentrated using the procedure described in the next section, for the purpose of purifying the enzyme.

Concentration of cell-free extract. After harvesting cells from the fermentor, the cell-free supernatant, containing alginase, was first concentrated at 4° C. by running it through Pellicon XL concentration device (Millipore) supplied with 10 kDa MW cut-off PGCLC10 membranes (Millipore, Piscatway, N.J.), then immediately exchanged with 20 mM PIPES buffer, pH 6.8. It is important to note that only de-ionized water (DI H₂O) was utilized during the process of concentration.

Ammonium sulfate precipitation. Previous experiments on precipitating alginase with ammonium sulfate determined that maximum alginase activity was detected at 70% fraction (Chakravorty 1998). Therefore, alginase preparation was precipitated with 70% saturated ammonium sulfate at 4° C. with constant stirring. The solution was allowed to equilibrate for 1 hr at 4° C. before centrifugation. The precipitate was then collected by centrifugation at 10000×g for 45 min at 4° C. and re-suspended in 20 mM PIPES buffer, pH 6.8.

Dialysis. The enzyme preparation was transferred into Spectrapor membrane with Mw cut-off 6000-8000 (Spectrum Laboratories, Inc.) and dialyzed against 20 mM PIPES buffer, pH 6.8, at 4° C. for 12 hrs with constant stirring to remove the ammonium sulfate from the enzyme preparation.

Ultra-filtration/Final concentration. The dialyzed enzyme solution was ultra-filtered and concentrated using Centriplus YM-10 Centrifugal filter; a device containing 10 kDa cut off regenerated cellulose membrane (Amicon Bioseparation, Millipore Corp, Bedford, Mass.). In this process, the sample was placed in the concentrator's reservoir, and then the device was centrifuged for 2 hrs at 3000×g and 4° C. The Centriplus YM-10 retentate (concentrate) was the final alginase concentrate used for the experiments in the next section.

At each step of purification or concentration, a sample was taken and frozen for later determining alginase activity, total protein, specific activity and percentage yield, to assess the effectiveness of the purification process.

The next sets of experiments were all carried out using the last preparation of concentrated alginase enzyme, the Centriplus YM-10 alginase concentrate.

Alginase concentrate was analyzed by discontinuous 12% (wt/v) sodium dodecyl sulfate polyacrylamide get electrophoresis (SDS-PAGE), according to standard procedures (Laemmli 1970). For molecular weight determination, 12% (wt/v) SDS-PAGE mini-gel was loaded with the following: 20 μl of broad-range unstained protein marker (6.5 to 200 KDa, Bio-Rad 161-0314), and 200 μl of Centriplus retentate. Gel was run for 5 hrs 200 volts, at room temperature. SDS— gel was stained with silver stain according to Bio-Rad protocol at current of 0.1 Amp. Alginase bands were identified by comparing SDS bands to the ones that showed activity in zymogram gel (described below).

To detect the activity of the alginase preparation, proteins of the alginase concentrate were separated by 12% native-PAGE, run for 5 hrs at 200 volts and constant current of 0.1 Amp. The alginase-containing native-PAGE were overlaid on zymogram gels, 8% native polyacrylamide containing 0.1% alginic acid, and incubated for 16 hrs in 20 mM Pipes buffer at room temperature. After incubation, the zymogram gels were stained with 0.08% (wt/v) toluidine blue-O in 7% (v/v) glacial acetic for 30 min. After decanting the stain, gels were de-stained in D.I. H₂O for 30 min and observing the activity bands. Toluidine blue non-specifically binds the non-degraded alginic acid (Langille 1996). Thus, the activity bands were unstained.

Activity of the purified alginase was assayed by the DNSA method at 5, 10, 20, 25, 37, and 55° C. Aliquots of 0.3 ml of the alginase concentrate were mixed with 0.7 ml of 0.5% alginate, pH 7.0, and incubated at the above mentioned temperatures for 30 min. Alginase activity was then determined by the DNSA method described previously.

Aliquots of alginase concentrate were incubated with 0.5% alginate, pH 7.0, in test tubes at 25° C. At 5 minute interval, reaction was stopped by boiling the reaction mixture with DNSA reagent for 5 minutes. The reaction mixtures were then cooled in cold water. Absorption was then measured at 575 nm.

Aliquots of the alginase concentrate in 20 mM PIPES buffer, pH 6.8, were equilibrated to 40, 50 and 60° C. in a water bath for 12 hrs. At certain time points, the heat-treated alginase samples were transferred to a chilled water bath. The residual activity was immediately determined using the DNSA procedure as previously described.

Alginase concentrate was dispensed in 0.5 ml aliquots and divided into three sets for determination of the enzyme shelf life at room temperature (25° C.), 4° C., and −20° C. The duration of the experiment was 60 days. Alginase activity was determined during the storage time using the DNSA method.

To determine the relative affinity if the alginase for its substrate, Michaelis-Menten constant was determined using the alginase concentrate, the Centriplus YM-10 concentrate. Aliquots 100 μl of alginase concentrate, contains approximately 86 □g protein, were mixed with alginic acid at concentration from 0.1 to 1.0% and incubated at 25° C. and alginase activity was monitored over a period of 2 hrs. Reaction initial rate, K_(m) and V_(max) were calculated.

To identify the alginase-encoding genes, 2-40's genomic sequence was surveyed for alginase genes using the protein sequence of alginases determined in other alginase-producing organisms. This was accomplished by utilizing the data base from the NCBI, National Center for Biotechnology Information⁴, using protein query-translated database, tblastn, of the BLAST⁵ algorithm, Basic Local Alignment Search Tool, (Altschul et al., 1990, 1994 and 1997, Karlin and Altschul 1990 and 1993,) at the NCBI. ⁵ BLAST^(®) (Basic Local Alignment Search Tool) is a set of similarity search programs, developed at NCBI, designed to explore all of the available sequence databases regardless of weather the query is protein or DNA.

After finding alginases in the 2-40 genome, the protein sequence of each alginase was analyzed using SMART⁶ (Simple Modular Architecture Research Tool) for the identification and annotation of genetically mobile domains and the analysis of domain architectures (Letunic et al., 2002, Schultz et al., 2000). These domains were annotated with respect to the functional class, tertiary structures and functionally important residues. Finally, using The Expert Protein Analysis System, ExPASy⁷, the molecular weight and pl of each alginase were determined. ⁷ The ExPASy (Expert Protein Analysis System) proteomics server of the Swiss Institute of Bioinformatics (SIB) is dedicated to the analysis of protein sequences and structures as well as 2-D PAGE.

Results

2-40 was grown in minimal media supplemented with 0.2% of alginate, fructose, galactose, glucose, lactose, sorbitol, or xylose. The cultures were incubated for 32 hrs at 25° C. with aeration. Growth was monitored by measuring the optical density (OD) at 600 nm, and enzyme activity (μg reducing sugar/ml) was determined by the DNSA protocol.

The lag phase lasted 4 hours for all cultures growing in each of the seven carbon sources. The log phase lasted 9 hrs in fructose, galactose, lactose, sorbitol and xylose, and 13 hrs in both alginate and glucose (FIG. 10). Decline phase did not start before 32 hrs when cultures were grown with alginate, glucose, fructose, lactose, or xylose as the main carbon source, while it started at the 28^(th) hr in case of galactose and as early as the 24^(th) hr in case of sorbitol. The decline phase in sorbitol was also steeper than the other carbon sources.

Alginase activity was detected in the spent media after 4 hrs in all the carbon sources. Alginate induced the production of 615 units of alginase activity while xylose induced 457 units at 32 hrs in the spent media.

To analyze alginase activity as a function of carbon source, alginase activity was fitted to the following equation: y=a+bx, where, y: is alginase activity, a: is intercept, b: is slop and x: is time (FIG. 26 and Table 3.1a). Analysis showed that time (T) explained 69% of the variations, while carbon source (S) and the interaction of carbon source with time (S*T) explained 23% and 8% of the variations, respectively (Table 3.1b). Statistics were not applied to sort out the time variable, however, since it was fully expected that alginases would accumulate with time. There was some enzyme activity loss which becomes apparent during the late stationary and decline phases of growth. One possibility is that enzymes are slowly degraded over time, initially more slowly than production. In fact, some protease actively was reported in 2-40 previously (Chakravorty 1998). The “F” values determine the variation significance according to the F distribution critical values table (Moore 1995). The overall means for alginase activity, regardless of time, for each carbon source were also calculated (Table 5.1)

TABLE 5.1 Overall means (±SE) of alginase activity as function of carbon source in 2-40 growth medium. Carbon source Alginate Galactose Glucose Fructose Lactose Sorbitol Xylose Mean* 332.52^(A) 173.89^(D) 86.70^(G) 137.04^(F) 162.89^(E) 176.78^(C) 250^(B) *Means with the same letter are not significantly different at Pr < 0.05, with Tukey Test. SE (Standard Error) = 0.421

To identify the best carbon source for alginase production, alginate, glucose and xylose were tested for their effect on alginase yield by growing 2-40 in minimal media supplemented with (wt/v) 0.2% of either of alginate, glucose, or xylose for 48 hrs at the same growth conditions described above. Growth measurements showed that decline phase began after 36 hrs in all the three carbon sources. Alginase activities in the supernatant neither increased nor decreased between 32 and 36 hrs of growth, however (unexpectedly) started to significantly decrease after 36 hrs. Results also showed that 36 hrs was the peak harvest time for alginase activity for 2-40 grown in alginate and xylose and 29 hrs when 2-40 was grown in glucose. The yield was also very different: alginate, 693 units of activity; xylose, 506 units; glucose 151 units (FIG. 11).

These results were subject to statistical analysis. A curve linear relationship was suggested to fit the relation between alginase activity and time as follows: y=a +b₁ x+b₂ x², where, y is alginase activity, a is intercept, b₁ and b₂ are partial regression coefficients and x is time. Briefly, these results showed that alginase yields were statistically different depending on the substrate, and that time of harvest was the most important variable. FIG. 11 a shows the effect of growing 2-40 in alginate, glucose or xylose, as the main carbon source, on alginase activity over a period of 48 hrs. The maximum alginase activities obtained in the three carbon sources were significantly different, and that the highest alginase activity was in the alginate medium at 36 hrs, and this was statistically valid (Table 3.2) as was the finding that carbon source (S), time (T), and the interaction between the two variables (S*T) explained 42%, 47% and 11% of the variations, respectively (Table 5.2a). The overall means for alginase activity for each of the three carbon sources were also calculated (Table 5.2b).

Analysis of the effect of Alginate, Glucose and Xylose as the main carbon source in the growth medium on alginase activity.

TABLE 5.2a ANOVA table for alginase activity as a function of carbon source (S), time (T), and their interaction (T * S) in 2-40 growth medium. Source DF SS SS %^(a) Mean Square F Value^(b) S 2 2832675 42 1416337 79592 Error I 6 107 0.001 17.795 T 12 3213645 47 267803 91557 Linear T 1 2242200 (32) 2242200 766564 Quadratic T 1 773372 (11) 773372 264401 S * T 24 772705 11 32196 11007 Error II 72 210.564 0.003 2.925 Corrected 116 6819344 100 Total Source: source of variations, DF: Degrees of freedom, SS: Sum of Squares, Coefficient of variation = 0.664054, R² = 0.999969 ^(a)Sum Square % = (SS Variable/SS Total) * 100 ^(b)F values are significant at P < 0.0001

TABLE 5.2b Overall means (±SE) of alginase activity of alginate, glucose and xylose as the main source of carbon in the 2-40 growth medium. Carbon source Alginate Glucose Xylose Mean* 475.15^(A) 98.54^(C) 337.54^(B) *Population mean, means with the same letter are not significantly different at Pr < 0.05, with Tukey Test. SE (Standard Error) = 0.1043

TABLE 3.2 Intercept (a), partial regression coefficients (b₁ and b₂), maximum alginase activity as a function of carbon source in 2-40 growth medium. Carbon Sources Alginate Glucose Xylose A  −75.43  −39.62  −72.08 b₁  42.22  12.96  31.53 b₂  −0.58  −0.22  −0.43 Max alginase  693^(A)  151^(C)  506^(B) activity* Time of max.  36.39  29.45  36.66 activity R²   0.9585   0.8630 0.9258 Cost: $/Liter   1.013   2.07 0.999 Cost: $/1000   1.46  13.7 1.97 units *Maximum activities were analyzed with t-test, activities with the same letters are not significantly different at DF = 74 and P < 0.05 Cost: all costs are in USD.

The effect of alginate concentration, as the main source of carbon, on growth and enzyme production was investigated by growing 2-40 in the minimum medium supplemented with alginate at concentrations (wt/v) of 0.1-0.6% and determining the enzyme activity at each concentration. Maximum activity was observed at 36.8 hrs in alginate concentrations of 0.5% and 37 hrs at concentration 0.6% with no significant increase in the activity at 0.6% (difference was analyzed with t-test). In fact, alginase production reached 1019 units at 0.5% and 1012 units at 0.6% (concentrations of more than 0.5% increased viscosity leading to reduced aeration). Moreover, the alginase production curves at both 0.5% and 0.6% were very similar. Since both growth and alginase activity increased with increasing alginate concentration up to 0.5%, this concentration was deemed to be the optimal as was 32 h of incubation, 25° C. and 200 rpm agitation, (FIG. 12).

For prediction of alginase production of 2-40 as a function of alginate concentration over the period of 48 hr the following quadratic equation was used: y=a+b ₁ x+b ₂ x ², where y: alginase activity, a: intercept, b₁ and b₂ are the graph partial regression coefficients for each concentration curve, and x: time. Alginase production was fitted to the above formula, with R² value of 0.94, indicating the appropriateness of the chosen formula. FIG. 24 and Table 3.3 depict the effect of alginate concentration on alginase production over the incubation period. Table 3.3 shows that alginate concentrations varied in intercept, ranging from −87.42 (at 0.5% alginate) up to −47.02 (at 0.1% alginate). This resulted in reaching maximum alginase activity at different time points for each alginate concentration. Analysis of variance illustrated that 79% of the variations were attributed to time, while 16% were attributed to alginate concentration, underscoring the importance of time as a significant factor in alginase production. “F” values confirm the significance of variations attributed to both time and alginate concentration (Table 5.3a). The overall means for alginase activity, regardless of time, for each concentration were also calculated (Table 5.3b). Tables 5.3a and b—Analysis of the effect of alginate concentration on alginase activity.

TABLE 5.3a ANOVA table for alginase activity as a function of alginate concentration (C), incubation time (T), and their interaction (C * T) in 2-40 growth medium. Source DF SS SS %^(a) Mean Square F Value^(b) C 5 3859829 16 771966 36760 Error I 12 249 0.001 21 T 12 19381397 79 1615116 209755 Linear T 1 14450075 (59) 14450075 1876633 Quadratic T 1 4231089 (17) 4231089 546492 C * T 60 1089846 4.5 18164 2359 Error II 144 1108 0.004 7.7 Corrected 233 24332430 100 Total Source: source of variations, DF: Degrees of freedom, SS: Sum of Squares, Coefficient of variation = 9.176513, R²= 0.999954 ^(a)Sum Square % = (SS variable/SS Total) * 100 ^(b)F value is significant at P < 0.0001

TABLE 5.3b Overall means (±SE) of alginase activity as function of alginate concentration in 2-40 growth medium. Alginate concentration (%) 0.1 0.2 0.3 0.4 0.5 0.6 Mean* 338.67^(E) 474.90^(D) 532.31^(C) 615.21^(B) 701.72^(A) 700.13^(A) *Population Mean, means with the same letter are not significantly different at Pr < 0.05, with Tukey Test. SE (Standard Error) = 0.0711

The 0.5% alginate minimal medium was supplemented with casein, yeast extract, or peptone at concentrations from 0.0 to 2 g/l. Activity was monitored every 6 hours during 54 hours of incubation. Alginase activity (in the supernatant) was maximum between 24 to 36 hrs, during stationary phase, after which enzyme activity declined slightly in the casein medium, and dramatically in YE and peptone media. In 0.2% YE, alginase activity peaked at 34 hrs with 1162 units. In 0.2% peptone, alginase activity was 1149 units at 34.36 hrs. In 0.2% casein, maximum alginase activity reached 1064 units at 34.98 hrs (FIG. 13). Without any supplement to the alginate minimal medium, alginase activity was 965 units at 34 hrs. For prediction of alginase production of 2-40 as a function of casein, peptone or yeast extract concentration, the following quadratic equation was used: y=a+b ₁ c+b ₁₁ c ² +b ₂ t+b ₂₂ t ², where y is alginase activity, a is the intercept, c is growth factor concentration, t is time, b₁, b₁₁, b₂ and b₂₂ are partial regression coefficients.

The above mentioned quadratic equation was used to analyze the observations of alginase production as a function growth factor type and concentration over the period of 54 hrs. These analysis validated alginase production as a variable of casein concentration (FIG. 25 a, and table 5.4a), peptone concentration (FIG. 25 b, Table 5.4b), and yeast extract concentration (FIG. 25 c, Table 5.4c) with time. Analysis of variance (Table 3.4) showed that, again, 93% of the variations were attributed to time (T), 0.05% to the growth factor type (S), and 3% to the growth factor concentration (C). However, the “F” values illustrated that each of these variables are indeed significant. Moreover, analysis showed that maximum alginase activity was induced in a concentration of 0.2% for all three substrates. In fact, analysis showed that further increase in the casein and yeast extract concentrations over 0.2% decreased the alginase activity, and in the case of peptone, increase in the concentration over 2% did slightly increase alginase activity; however according to t-test analysis this increase is statistically insignificant. The maxima of alginase activity as variable of the three substrate concentrations were analyzed using t-test. These showed that alginase activity was significantly higher in 0.2% yeast extract than in the same concentration of casein or peptone (Table 3.5).

5.4 Analysis of the effect of growth factor in the growth medium on alginase activity.

TABLE 5.4a Maximum alginase activity of 2-40 when grown in casein as a growth factor in the growth medium. Casein Concentration (%) 0 0.05 0.1 0.15 0.2 Max activity* 919 989 1037 1062 1064 Time at max activity 34.98 34.98 34.98 34.98 34.98 R² = 0.9335 *Maximum alginase activities at 0.15 and 0.2 were analyzed wit t-test and the difference was found significant at DF = 56, and P < 0.05

TABLE 5.4b Maximum alginase activity of 2-40 when grown in peptone as a growth factor in the growth medium. Peptone Concentration (%) 0 0.05 0.1 0.15 0.2 Max activity* 973 1035 1085 1123 1149 Time at max activity 34.36 34.36 34.36 34.36 34.36 R² = 0.9140 *Maximum alginase activities at 0.15 and 0.2 were analyzed wit t-test and the difference was found significant at DF = 56, and P < 0.05

TABLE 5.4c Maximum alginase activity of 2-40 when grown in yeast extract as a growth factor in the growth medium. Yeast Extract Concentration (%) 0 0.05 0.1 0.15 0.2 Max activity* 1003 1071 1119 1150 1162 Time at max activity 33.94 33.94 33.94 33.94 33.94 R² = 0.9217 *Maximum alginase activities at 0.15 and 0.2 were analyzed wit t-test and the difference was found significant at DF = 56, and P < 0.05

TABLE 3.4 ANOVA table for alginase activity as a function of growth factor (S), growth factor concentration (C), time (T), and their interactions (S * C, S * T, and T * C) Mean F Source DF SS SS %* Square Value^(a) S 2 29048 0.05 14523.896 7.69^(b) C 4 1972561 3.22 493140 261 Linear C 1 1876352 (3.06) 1876352 731 Quadratic C 1 35669 (0.05) 35669 14 S * C 8 100051 0.16 12506 6.62 Error I 30 56669 0.09 1889 0.74^(c) T 9 56986991 93 6331888 2466 Linear T 1 29174527 (47)    29174526.63 11364 Quadratic T 1 25544774 (42)    25544774 9950 S * T 18 512786 0.8 28488 11 T * C 36 637381 1 17705 6.9 Error II 342 877992 1.4 2567 Corrected 449 61173480 100 Total Source: source of variations, DF: Degrees of freedom, SS: Sum of Squares, Coefficient of variation = 7.314432, R² = 985648 * SS % = (SS variable/SS Total) * 100 ^(a)All F values are significant at P < 0.0002, unless otherwise noted. ^(b)F value is significant is significant at P = 0.002 ^(c)F value is significant is significant at P = 0.8446

TABLE 3.5 T-test of maximum alginase activities obtained when casein, peptone, or yeast extract was added to 2-40 medium as growth factor. Yeast Casein Peptone Extract Max alginase 1064 1149 1162 activity Time at max 34.98 34.36 33.94 activity Concentration 0.2% 0.2% 0.2% at max activity (%) R² 0.9335 0.914 0.9217 Cost: $/Liter 1.44 1.28 1.58 Cost: $/1000 1.35 1.11 1.35 units Maximum alginase activities of casein, peptone and yeast extract were compared with t-test and the differences in alginase activity were found significant at DF = 56, and P < 0.05 Cost: all costs are in USD.

2-40 is a marine bacterium requiring sea salts. Instant Ocean (IO), a mixture of sea salts, was applied in the minimal medium at concentrations of 0.1, 2.3, 3.5, 5, and 7%. 2-40 grew in a wide range of salt from 1-5%, with slower growth at 7% (FIG. 14). Maximum alginase activities were detected between 38-39 hours in 2.3-3.5% IO, 1180-1252 units. Alginase yields at 2.3% and 3.5% IO were analyzed by t-test and difference found to be significant. Additionally, since growing 2-40 in 3.5% IO would inhibit the growth of some contaminant microorganisms (e.g. Bacillus sp.), this concentration was applied in subsequent experiments. For prediction of alginase activity as a function of instant ocean concentration, alginase activity was fitted to a quadratic equation over time and represented by the formula: y=a+b₁x+b₂x², where y is alginase activity, a is intercept, b₁ and b₂ are the graph partial regression coefficients, and x is time.

To analyze the effect of Instant Ocean (IO) concentration on alginase production by 2-40, alginase activity was fitted to a quadratic relationship, with R² ranging from 0.9151 to 0.9631 (Table 3.6). Analysis showed that the IO concentration affected alginase activity, with alginase activity reaching a maximum concentration at different time points (FIG. 24 and Table 3.6). A T-test was used to compare the two highest alginase activity maxima which were obtained in 2.3% and 3.5% IO. T-test showed that 3.5% IO supported significantly higher alginase yield than 2.3% IO did and so the statistical analysis was particularly revealing in this case. Table 5.5a, shows the analysis of variance of alginase activity as affected by IO concentration and incubation time. This analysis reveals that 25% of variations can be attributed to IO concentration (C), 67% to incubation time (T) and 7% to the interaction of IO concentration with time (C*T). Moreover, “F” values showed the significance of variations attributed to IO concentration and time. The overall means for alginase activity, regardless of time, for each instant ocean concentration were also calculated (Table 5.5b).

5.5 Analysis of the effect of Instant ocean concentration on alginase activity.

TABLE 5.5a ANOVA table for alginase activity as a function of Instant Ocean concentration (C), time (T), and their interaction (C * T) in 2-40 growth medium. F Source DF SS SS %^(a) Mean Square Value^(b) C 4 7773734 25.5 1943433 95033 Error I 10 204 0 20.45 T 12 20569370 67.5 1714114 480144 Linear T 1 17085204 56 17085204 4785771 Quadratic T 1 2721886 9 2721886 762433 C * T 48 2130499 7 44385 12433 Error II 120 429 0.002 3.57 Corrected 194 30474236 100 Total Source: source of variations, DF: Degrees of freedom, SS: Sum of Squares, Coefficient of variation = 9.176513, R² = 0.999986 ^(a)SS % = (SS variable/SS Total) * 100 ^(b)F values are significant at P < 0.0001

TABLE 5.5b Means (±SE) of alginase activity as function of instant ocean concentration. IO concentration (%) 1 2.3 3.5 5 7 Mean* 450.46^(D) 803.15^(B) 848.64^(A) 510.82^(C) 342.48^(E) Means with the same letter are not significantly different at Pr < 0.05, with Tukey Test. SE (Standard Error) = 0.0485

TABLE 3.6 Intercept (a), partial regression coefficients (b₁ and b₂) for alginase activity as a function of Instant Ocean concentration in 2-40 growth medium. Instant Ocean (%) 1% 2.3% 3.5% 5% 7% a −51.30 −112.48 −105.47 −104.56 −91.17 b₁ 35.19 67.56 68.82 38.59 31.53 b₂ −0.43 −0.88 −0.87 −0.39 −0.40 Maximum 671.23 1180.89 1252.41 853.72 524.29 activity* Time at max Y 41.07 38.29 39.46 49.66 39.04 R² 0.959 0.9584 0.9631 0.9444 0.9152 Cost: $/liter 1.53 1.575 1.61 1.64 1.69 Cost: $/1000 2.28 1.33 1.28 1.92 3.22 units Maximum alginase activity at both 2.3% and 3.5% were analyzed by t-test, and difference between the two values was found significant at DF = 74 and P < 0.05 Cost: all costs are in USD.

In the previous experiments, glucose (G) induced rapid biomass increase, while alginate (A) was the best alginase inducer. Therefore, a combination of these two carbon sources was tested as a way to achieve highest alginase yield. The tested % A: G % (wt/v) ratios were: 0.5A:0.0G, 0.45A:0.05G, 0.40A:0.10G, 0.35A:0.15G, and 0.30A:0.20G (plus 3.5% 10 and 0.2% YE). A combination of 0.45% alginate and 0.05% glucose supported 1348 units of alginase at 40 hrs, which is 119 units more than the medium containing 0.5% alginate alone without glucose (FIG. 15). Increasing the glucose concentration, while decreasing alginate concentration delayed alginase production. With a combination of 0.4% A:0.1% G, alginase activity was not detected until 16 hrs and by further increasing glucose concentration to 0.15% (decreasing alginate concentration to 0.35%) detectable alginase production was delayed until 20 hrs. At 0.2% glucose (0.3% alginate), alginase activity was not detected for 24 hrs.

For prediction of alginase activity as a function of alginate/glucose combination, alginase activity was fitted to a quadratic equation over time and represented by the formula: y=a+b₁ x+b₂ x², where y is alginase activity, a is intercept, b₁ and b₂ are the graph partial regression coefficients, and x is time.

The effect of growing 2-40 in varying Alginate/Glucose combinations (% A/% G) on alginase activity was fitted to a linear relationship over time (FIG. 15 a), with R² ranging between 0.9072 and 0.9736 (also see Table 5.6a). Analysis of these data supported the initial observation that different percentage combinations were significant with respect to alginase production (Table 5.6a). Within the studied incubation period, the combination of 0.45% A/0.05% G induced 1476 alginase units at 42 hrs, which was higher than that induced by 0.5% A/0% G which was 1229 units at 43 hrs. Other A/G combinations induced even higher alginase activities, however beyond the studied incubation period. For instance, 0.4% A/0.1% G induced 1563 alginase units at 62 hrs of incubation, and 0.35% A/0.15% G required 140 hrs to induced 1936 alginase units. Alginase production in both 0.5% A/0% G and 0.45% A/0.05% G were compared with t-test and the difference was found significant. “F” values showed that variations caused by A/G combinations and time were significant (see Table 5.6b).

TABLE 5.6a Intercept (a), partial regression coefficients (b₁ and b₂) for alginase activity as a function of alginate/glucose mix ratio (A/G) A %/G % Combinations 0.5A/ 0.45A/ 0.4A/ 0.35A/ 0.3A/ 0.0G 0.05G 0.1G 0.15G 0.2G a −69.84 −275.45 −239.31 −154.32 −115.55 b1 60.1302 82.5299 57.8239 29.6615 19.6454 b2 −0.6956 −0.9724 −0.4638 −0.1052 −0.2610 Maximum 1229 1476 1563 1936 254 activity (y) Time of max 43 42 62 140 38 activity (x) R² 0.9736 0.9072 0.9157 0.9424 0.9578 Maximum alginase activities obtained in 0.5A/0.0G and 0.45A/0.05G were analyzed with t-test and the difference between the two combinations was found significant at DF = 74 and P < 0.05.

TABLE 5.6b ANOVA table for alginase activity as a function of alginate/glucose mix ratio (A/G) in 2-40 growth medium. Source DF SS SS %^(a) Mean Square F Value^(b) (A/G) 4 3221196 5.6 805299 55538 Error I 10 145 0 14.5 T 12 51507752 89 4292313 255.57 Linear T 1 47594980 (82.7) 47594980 2834 Quadratic T 1 958480 (1.67) 958480 57 Error II 168 2821596 5 16795 Corrected 194 57550689 100 Total Source: source of variations, DF: Degrees of freedom, SS: Sum of Squares, Coefficient of variation = 17.38089, R² = 0.950972 ^(a)SS % = (SS variable/SS Total) * 100 ^(b)F values are significant at P < 0.0001, except where otherwise mentioned ^(c)F value is significant at P = 1.0 Scale-up of alginase production of 2-40

An optimum medium composition, shown in Table 3.1, was used for the remainder of the experiments because experiments showed that a medium (Alginase Production Medium, APM) composed of: 0.05% glucose, 0.45% alginate, 3.5% sea salts, and 0.2% Yeast extract, pH 7.6 enhanced alginase production nearly two fold (1354units vs. 693 units, a 95% increase, Table 3.8) more than the preliminary minimal medium. In APM, the lag phase was 8 hrs, the log phase lasted 12 hrs with generation time of 3.68 hr. Stationary phase was reached after 20 hrs, and lasted for 12 hrs after which the decline phase began. The most productive time for alginase harvest was, in fact, at 39 hr, 1355 alginase units at the beginning of the decline phase (FIG. 28 and Table 3.7). This experiment served as a preparatory step for the scale-up experiment of alginase production.

It was postulated that the oxygen limitations of the shake flask would be minimized using a stirred fermentor, with stirring at 400 rpm, and aeration at 6000 cc/min and temperature at 25° C. In APM, the lag phase was 4 hrs, the log phase lasted 16 hrs with generation time of 2.3 hr. Stationary phase was reached after 20 hrs, lasting for 12 hrs after which the decline phase began. The most productive time for alginase harvest was, in fact, at 36 hr, which yielded 1690 alginase units at the beginning of the decline phase. Under these conditions, and after 36 hrs, 2-40 total cells registered an OD of 1.85. I. Growth and alginase production of this experiment are shown in FIG. 28 and Table 3.7. There was no pH control. The initial pH of the un-inoculated medium was 7.6 and the pH of the spent culture was 8.2.

FIG. 28 b compares the growth of 2-40 in the optimized alginase production medium (APM) in flask batch culture and in a fermentor. Alginase activity was fitted to a linear relationship with time with R² value of 0.9811 for the flask and 0.9560 for the Fermentor (Table 5.7). Data analysis showed the maximum alginase activity was reached in shorter time in the case of Fermentor (1690 alginase units at 36 hrs) than in the case of the flask (1355 alginase units at 39 hrs). Analysis of variance of alginase activity showed that 89% of variations were attributed to time, while 3.6% of the variations were attributed to type of incubation vessel. “F” values showed that variations attributed to difference in the incubation vessel type were significant.

5.7 Analysis of the effect of growing 2-40 in flask or fermentor on alginase activity.

TABLE 5.7 ANOVA table for alginase activity as a function of incubation vessel (V), Flask vs. Fermentor, and their interaction (V * T) F Source DF SS SS %^(a) Mean Square Value^(b) V 1 873865.85 3.6 873865.85 40.45 T 12 21468786 89 1789065.52 82.81 Linear T 1 17129566 (71) 17129566 792.88 Quadratic T 1 3545159 (14.8) 3545159 164 V * T 12 502316 2 41859.71 1.94^(c) Error 52 1123423 4.7 21604 Corrected 77 23968391 100 Total Source: source of variations, DF: Degrees of freedom, SS: Sum of Squares, Coefficient of variation = 14.24759, R² = 0.953129 ^(a)SS % = (SS variable/SS Total) * 100 ^(b)F values are significant at P < 0.0001, except where otherwise mentionedis significant at P = 0.0508

TABLE 3.8 Optimization of 2-40 growth medium for alginase production. Alginase activity at Cost/liter Alginase peak time (μg (per 1000 Medium Type of peak time reducing % alginase # composition^(a,b) experiment (hr)^(c) sugar/ml/30 min)^(d) increase^(e) units)^(f) 1 0.2% Alg Shake 36 693 0 $1.01/L 0.1% YE Flask ($1.548) 2.3% IO 2 0.5% Alg Shake 37 1019 47 $1.39/L 0.1% YE Flask ($1.364) 2.3% IO 3 0.5% Alg Shake 34 1162 68 $1.576/L 0.2% YE Flask ($1.356) 2.3% IO 4 0.5% Alg Shake 39 1252 81 $1.606/L 0.2% YE Flask ($1.283) 3.5% IO 5 0.45% Alg + 0.05% Shake Flask 39 1476 113 $1.87/L Glu ($1.381) 0.2% YE 3.5% IO 6 0.45% Alg + 0.05% Fermentor 36 1690 143 $1.87/L Glu (Scale-up) ($1.107) (APM) ^(g) 0.2% YE 3.5% IO ^(a)medium ingredients are referred to as: Alg: Alginate, YE: Yeast Extract, IO: Instant Ocean, Glu: Glucose. ^(b)Ingredient shown in Bold indicates final modifications in medium composition. ^(c)peak time (time of maximum alginase activity) was calculated using the proper statistical analysis (discussed later). ^(d)Alginase activity compared with medium # 1, Alginase activity at peak time was calculated using statistical analysis. ^(e)percentage increase in alginase activity compared to that obtained from 0.2% alginate minimal medium. ^(f)cost per liter of medium included the cost of Tris-HCl and NH₄Cl. Cost was then divided by the alginase units produced to give the cost per 1000 units of alginase activity. All cost are in USD. ^(g)Alginase Production Medium (APM).

The alginase slurry purification criteria are shown in table 3.2. The fermentor's cell-free supernatant was concentrated, using the Pellicon XL concentration device (Millipore) fitted with 10 kDa MW cut-off PGCLC10 membrane (Millipore, Piscatway, N.J.), to 200 ml. This step increased the specific activity (μg reducing sugar/mg protein/ml) 10 fold. Ammonium sulfate precipitation, dialysis, and then ultra-filtration (10 kDa cut-off Mw), each further increased the alginase activity to a final total of 21× the alginase activity in the starting cell-free extract (Table 3.9).

TABLE 3.9 Purification of alginase and its specific activity. mg SA³ Purification Vol. μgRS/ Total units protein/ Total μgRS/mg Yield step (ml) ml¹ (×1000) ml² protein protein/ml (%) x-fold Cell-free 7300 1687 12315 0.78 5721 2153 100 1 extract Pellicon 7100 12 85 0.75 5335 16 0.69 0 XL⁴− Filtrate Retentate 200 31200 6240 1.44 288 21667 51 10 Ammonium 160 30125 4820 0.98 156 30897 39 14 Sulfate precipitate Dialysis 112 36852 4127 1.04 117 35273 34 16 Ultra-filtration⁵ 45 38650 1739 0.86 39 44590 14 21 ¹μg reducing sugar (RS)/ml, determined by DNSA standard method (see materials and methods). ²protein concentration was determined by BCA method (see materials and methods). ³Specific activity (SA) units calculated as μg/ml RS per mg/ml protein. ⁴cut-off Mw is 10k Da for pellicon XI membrane ⁵cut-off Mw is 10k Da for Ultra-filtration membrane.

Previous results showed that the most abundant alginate depolymerase has MW of 66 kDa (Chakravorty 1998). However, the present work showed that out of six different active alginases, the 58 kDa alginase (later to be identified in the genome annotation as AlgE) had the highest activity as demonstrated by the zymograms. The aim was to purify, concentrate, and study this alginase and the total alginase concentrate (ultra-filtrate, Table 3.9).

To identify and determine the molecular weights of the alginases, proteins in the alginase concentrate were first separated by 12% sodium dodecyl sulfate polyacrylamide get electrophoresis (SDS-PAGE), according to standard procedure (Laemmli 1970), and 12% native-PAGE. The native-PAGE was then overlaid on an 8% polyacrylamide gel containing 0.1% alginic acid and incubated for 16 hrs in 6.8pH PIPES buffer (see Materials and Methods). A comparison of the active bands revealed by the zymogram with those of the SDS-PAGE gel allowed the identification of six alginases. The molecular weights of these alginases, as determined by the SDS-PAGE, were 12, 56, 62, 81, 125 and 165 kDa (FIG. 19). The most active alginase was the 56 kDa, based on the loss of staining from the protein band in the zymogram.

To determine the optimum temperature for total alginase activity, aliquots of the alginase concentrate were incubated with 0.5% alginic acid for 30 min at 5, 10, 20, 25, 37, and 55° C. and alginase activity was assayed by the DNSA method. Alginase activity was optimum at a temperature range between 20 and 37° C., with maximum activity at 25° C. (FIG. 20). At elevated temperatures, alginase activity was reduced to 60% of the activity detected at 25° C. after 30 min. At temperature below 20° C., alginase activity dropped to 48% relative to the activity detected at 25° C.

Aliquots of alginase concentrate were incubated with 0.5% alginate, pH 7.0, at 25° C. First order kinetics for the first 30 min indicated that the DNSA was not substrate-limited over that interval. This is why the DNSA was determined after 30 min, (FIG. 3).

Aliquots of the alginase concentrate in 20 mM PIPES buffer, pH 6.8, were equilibrated to 40, 50 and 60° C. in water baths for 12 hrs. At intervals, alginase samples were withdrawn and cooled in ice and alginase remaining activity was assayed by the DNSA method. At 40° C., the mixed alginase slurry was more stable than at 50° C. which was more stable than 60° C. After one hour (FIG. 13), the alginase preparation lost approximately 15% of its activity at 40° C., 50% at 50° C. and 70% at 60° C. The hyperbolic denaturation curves suggest that one or more of the enzymes in the slurry were heat resistant.

To determine the shelf-life of the alginase concentrate, 0.5 ml aliquots were dispensed and divided into three sets of tubes. One set was stored at room temperature (25° C.), the second at 4° C., and the third at −20° C. All preparations were stored for up to 60 days. Several tubes were removed from each set at intervals and alginase activity was determined. Alginase was stable at −20° C. (FIG. 5). At 4° C., alginase retained 84% of its activity at the end of 60 days, while at room temperature; it retained less than 50% of its activity.

3.3.6 Alginase kinetics. The success of enzyme analysis depends to a great extent on the purity of the enzyme. Additionally, using too little; or too much; enzyme can also lead to analysis failure. However, appropriate amounts, of the partially purified enzymes, can also be analyzed (Lowry and Passonneau 1972). To determine the relative affinity of alginase for its substrate, the Michaelis-Menten constant was determined using the alginase concentrate. 100 μl, containing approximately 86 μg protein, were mixed with alginic acid at concentration from 0.1 to 1.0% and incubated at 25° C. Alginase activity was monitored over a period of 2 hrs. The reaction's initial rate, K_(m) and V_(max) were calculated. The relationship between the initial velocity, (v), of alginase and the concentration of alginic acid [S], the substrate, was determined by Michaelis-Menten plot, (FIG. 6). The data revealed that the maximum velocity, (V_(max)), was approximately 67.68 □g reducing sugar/min and the K_(m) was 0.0253 mM, suggesting that alginase has a high affinity for its substrate, alginate¹ Molecular weight of sodium alginate was obtained from Sigma, ranging from 12 kDa to 80 kDa. Hence the average, 48 kDa, was used in the calculation of K_(m) and V_(max).⁸ ⁸Molecular weight of sodium alginate was obtained from Sigma, ranging from 12 kDa to 80 kDa. Hence the average, 48 kDa, was used in the calculation of K_(m) and V_(max).

However, because of the hyperbolic shape, Michaelis-Menten plot made it difficult to extrapolate accurately to infinite substrate concentration in order to accurately calculate V_(max), and thus K_(m). Therefore, Lineweaver-Burk plot was constructed by converting the hyperbolic relationship of Michaelis-Menten equation into a linear function (Lineweaver and Burk. 1937). This was done by plotting the reciprocal of the initial velocity, 1/v, against the reciprocal of alginate concentration, 1/[S]. Hence, V_(max) and K_(m) were more precisely computed to be 90.09 μgRS/min and 0.054 mM, respectively (FIG. 7). These values are comparable to those determined for purified alginate lyases from other microorganisms (Table 3.10).

TABLE 3.10 K_(m) values for bacterial alginase compared to 2-40 aglinase Alginate (source) K_(m) V_(max) Ref 2-40 Macrocysts pyrifera 2592 mg/ml 90.09 □gRS/min This work (0.054 mM) Azotobacter M-alginate from P. aeruginosa. 0.46 mM NR Ertesv{dot over (a)}g vinelandii etal., 1998 Pseudomonas sp. I - A. vinelandii 1500 mg/ml NR Davidson et al., 1976 Pseudomonas sp. VIII - A. vinelandii 1850 mg/ml NR Davidson et al., 1976 Pseudomonas sp. IV - A. vinelandii 2460 mg/ml NR Davidson et al., 1976 Pseudomonas sp. V - A. vinelandii 2180 mg/ml NR Davidson et al., 1976 Pseudomonas sp. VII - A. vinelandii 4400 mg/ml NR Davidson et al., 1976 A. chroococcum Macrocysts pyrifera 0.08 mM 183 □g/min Peciña et al., 1999 AlxM_(B) from M. pyrifera alginate 0.011 mM 141 □mol/min Chavagnat et recombinant E. coli al., 1998 AlxM_(B) from M-blocks¹ 0.60 mM 139 □mol/min Chavagnat et recombinant E. coli al., 1998 AlxM_(B) from pentamannuronate 0.180 mM 103 □mol/min Chavagnat et recombinant E. coli al., 1998 Klebsiella Poly-mannuronate (in 0.059 mg/ml 0.019 AU/min² Haugen et al., aerogenes 0.05M Tris buffer) 1990 Haliotis sp. Poly-mannuronate (in 0.052 mg/ml 0.026 AU/min² Haugen et al., 0.05M Tris buffer) 1990 NR: Not reported ¹M-blocks: mannuronate blocks were prepared from bacteria alginates as reported by Heyraud et al., 1998. ²Enzymatic activity was reported as absorbance units (AU) per min

A draft of sequence of the 2-40 genome was obtained in conjugation with the United States Department of Energy Joint Genome Institute. To identify the genes encoding 2-40 alginases, the newly released 2-40 genomic sequence was compared to the sequences of 73 previously characterized alginase-producing microorganisms in the NCBI database. The program on choice was Basic Local Alignment Search Tool (BLAST). Eleven open reading frames were detected, namely AlgA, AlgB, AlgC, AlgD, AlgE, AlgF, AlgG, AlgH, AlgI, AlgJ and AlgK (Table 3.11). Amino acid sequences of each the 2-40 alginases were aligned with their best hit alginase from other bacteria and further annotated using the ClustalW alignment program (Thompson, et al., 1994).

The amino acid sequences of the alginases were analyzed by Simple Modular Architecture Research Tool (SMART) to determine the signal peptides, binding domains, repeats, motifs and other features (Tables 3.12 and 3.16 and FIG. 7).

TABLE 3.11 Alginases^(a) produced by 2-40: Mw, pl, and best sequence match using E values. Alginase MW E Percent gene AA (kDa)^(b) pl^(b) Best Hit^(c) Value^(d) Identity^(c) AlgA 345 37 6.83 Klebsiella 3e−62 47 pneumoniae AlgB 762 83 6.15 Pseudomonas sp. 5e−85 44 AlgC 738 81 5.53 Pseudomonas sp.  1e−171 44 AlgD 613 65 [0001] Klebsiella 1e−84 57 pneumoniae AlgE 524 56 [0002] Klebsiella 1e−96 63 pneumoniae AlgF 1554 163 4.39 Klebsiella 4e−60 49 pneumoniae AlgG 875 94 4.26 Corynebacterium sp. 2e−38 39 ALY-1 AlgH 894 93 4.13 Pseudomonas sp. 2e−46 30 AlgI 525 57 8.92 Pseudomonas sp. 6e−36 30 AlgJ 541 57 4.78 Pseudoalteromonas sp. 2e−86 67 IAM14594 AlgK 337 37 6.46 Vibrio halioticoli 3e−47 38 ^(a)signal peptides were detected by SMART, Simple Modular Architecture Research Tool. All alginases, except AlgA and AlgK, were determined to have signal peptide. ^(b)Molecular weight and pl are determined using the ExPASY program, ^(c)2-40 putative alginases were run against the database of the Computational Biology Program of the Life Sciences Division of Oak Ridge National Laboratory, results showed Best hit with its E value and percent identity. ^(d)E values: each value represents the number of sequences with a score greater-than, or equal to, X, expected absolutely by chance. E values are calculated using Hidden Markov Models.

AlgA is a 345 amino acid protein with a calculated Mw of 37 kDa (Table 3.11). It contains a 114 amino acid helicase superfamily c-terminal domain, termed HELICc. In general, this domain family is found in a wide variety of helicases and helicase related proteins. Such proteins normally function as a helicase, in ATP binding or nucleic acid binding. The following describes the domains shown in FIG. 7.

AlgB is a 762 amino acid with a calculated Mw of 83 kDa (Table 3.11). It contains a very interesting stretch of seven Parallel beta-helix (PbH1) repeats. These repeats are found in pectate lyases and rhamno-galacturonase A. Its conformation includes a stack of parallel beta strands that are coiled into a large helix. Each coil of the helix is a structural repeat. Proteins containing these repeats are, mostly, carbohydrases. No carbohydrate binding modules (CBM) were identified, possibly because: a) there aren't any, b) there were not found by annotation programs, possibly representing a previously unidentified CBM.

AlgC is a 738 amino acids protein with a calculated Mw of 81 kDa with a low compositional complexity region with sequence of LLGDGADGDQGAL (SEQ ID NO: 14). Perhaps importantly no CBM were detected. In carbohydrases that are part of a multi-array complex, the CBMs are found on the scaffolds and not in the catalytic proteins.

AlgD contains a 140 amino acid carbohydrate binding domain, RICIN, which is a beta-trefoil domain formed from presumed gene triplication. AlgD also contains an FA58C domain, a cell surface-attached carbohydrate-binding domain, and a 24 amino acid stretch of serine between positions 307 and 330 with sequence of [SSSSSSSSSSTSSTSSTSSTSSSS](SEQ ID NO: 15). The serine rich sequence is 146 amino acids removed from RICIN and 51 amino acids removed from a predicted active site region (discussed later).

AlgE contains a 39 amino acid domain, between positions 31 and 69 and composed of alternate threonine and proline with sequence of [TTPTPTPTPTPTPTPTPTPTPTPTPTPTPTPTPTPTPTP](SEQ ID NO: 16). This depolymerase also contains a 135 amino acid FA58C domain between positions 71 and 205. A region of low compositional complexity was also found between positions 207 and 230 with sequence of ETGTPTEDPVVVEPPEPPAPTDGD (SEQ ID NO: 17).

AlgF, the biggest of all eleven 2-40 alginate depolymerases, is composed of 1554 amino acids and has a calculated molecular weight of 163 kDa. It contains 9 repeats of PbH1 (Parallel beta-helix), described above. Three regions of low compositional complexity were detected, the first between positions 759 and 777 with sequence ANGLLNDANSLAGANASAL (SEQ ID NO: 18), the second between positions 1074 and 1095 with sequence PVEPGNGEDEGNGGTTTEVTDG (SEQ ID NO: 19), and the third between NO: 19), and the third between positions 1122 and 1133 with sequence GTVVVTDGVTIT(SEQ ID NO: 20).

AlgG, the second largest alginate depolymerases of 2-40, contains a 264 amino acid FA58C domain (described above). This putative depolymerase also contains two repeats of the Polycystic Kidney disease (PDK) domain. These domains contain 14 repeats and are present in microbial collagenases. A 133 amino acid domain, belonging to the CBM-4-9 carbohydrate binding family, was detected between positions 480 and 612 of the protein. The CBM-4-9 family includes diverse binding domains, attaching to several different polysaccharide conformations.

AlgH contains a 47 amino acid region of low compositional complexity starting from position 25 and ending at position 71. This region is rich in proline, glycine and glutamic acid (EGEP). The sequence of this region is PDPDPDPIEEPEGEPEGEPEGEPEGEPEGEPEGEPEGEPEGEPEGEP (SEQ ID NO: 21) AlgH also contains 4 Parallel beta-helix repeats (described above) ranging between 22 and 32 amino acid long. A low compositional complexity region is located between positions 516 and 531 with sequence of DLTAAAADTGDFMVT(SEQ ID NO: 22). AlgH also contains a 168 amino acid domain of the CBM-4-9 protein family.

AlgI contains a domain of the pectin lyase-like protein superfamily, with two representations, due to overlapping domains. In the first representation, this domain is 345 amino acid-long and located between positions 38 and 382. It has a single-stranded right-handed beta-helix with each turn made by 3 strands with short links duplication and the turns of the helix are structural repeats. In the second, the domain is 276 amino acid-long and located between positions 36 and 312.

AlgJ contains a 122 amino acid CBM-4-9 domain starting at position 10 and ending at position 131 (described above). It also contains a 142 amino acid FA58C domain starting at position 144 and ending at position 285 (described above). AlgJ also contains a 22 amino acid region of low compositional complexity with a repeating sequence of Threonine-Proline (TP), starts from position 290 and ends at position 311. The sequence of this region is: TPTPTPTPTPTPTPTPTPTPTP (SEQ ID NO: 23).

AlgA and AlgK were the smallest of the eleven alginases. No CBM were identified by the SMART analysis.

3.6. Alginases: Unusual domains

AlgD has a Ricin domain. RICIN is a legume lectin from the seeds of the castor bean plant Ricinus communis (Rutenber et al., 1987). Primary structure analysis has shown the presence of a similar domain in many carbohydrate-recognizing proteins like plant and bacterial AB-toxins and glycosidases. This domain, known as the ricin B lectin domain, can be present in one or more copies and has been shown in some instance to bind simple sugars, such as galactose or lactose. The ricin B lectin domain is composed of three homologous subdomains of 40 amino acids (alpha, beta and gamma) and a linker peptide of around 15 residues (lambda). It has been proposed that the ricin B lectin domain emerged from gene triplication from a primitive 40 residue galactoside-binding peptide (Hazes 1996). The most distinct sequence feature is the presence of a Q−W pattern. Moreover, ricin B lectin domain has been referred to as (Q×W)₃ (SEQ ID NO: 24) domain since it contains three homologous Q×W repeats, some of which contain a conserved disulfide bond. In the 2-40 alginases, this domain is believed to be a CBD, binding alginate to put another domain, the catalytic site, in proximity to the substrate.

FA58C is found in AlgD, E, G and L. It is also present in eukaryotes and assumed to have horizontally transferred to eubacterial genomes. This domain is found as a C terminal of Blood coagulation factors V and VIII (also called F5/8 type C, FA58C, or C1/C2-like domain), where it is composed of 150 amino acids and repeated twice. In these coagulation factors, the repeated domains compose part of a larger functional domain which promotes binding to anionic phospholipids on the surface of platelets and endothelial cells. The C-terminal domain of the second FA58C repeat (C2) of coagulation factor VIII has been shown to be responsible for phosphatidylserine-binding and essential for activity. It forms an amphipathic alpha-helix, which binds to the membrane. FA58C contains two conserved cysteine in most proteins, which link the outermost points of the domain by a disulfide bond. A related domain, named discoidin I-like domain, was found in slime mold, which shares a common C-terminal region of about 110 amino acids with the FA58C domain, but whose N-terminal 40 amino acids are much less conserved. Similar domains have also been detected in other extracellular and membrane proteins. In 2-40, it may be involved in protein-protein interactions.

PKD domains are present in AlgG. They were first identified in the Polycystic Kidney Disease protein 1 (PKD1) and are involved in adhesive protein-protein and protein-carbohydrate interactions. Most of these domains are found in the extracellular parts of proteins involved in interactions with other proteins. In 2-40 they could be involved in anchoring the protein to the surface of the cell, or act as CBD. They are present in polysaccharides from a member of other organisms where there is anecdotal evidence (in a few of many observations) that it disorders the crystalline part of the polymer making it more accessible to attack.

Carbohydrate-binding modules (CBMs) are a class of protein comprising 32 families classified on the basis of amino acid sequence similarity. CBMs can be grouped into 3 types based on their specificity for crystalline polysaccharides, Type A, glycan chains, Type B, or small soluble sugars, Type C.(Boraston 2003, personal communication).

TABLE 3.12 Alginases produced by 2-40: Stop codon, unusual domain, and amino acid repeats. Predicted Active AA Alginase Stop CBD^(a) MMBD^(b) active site site Repeat^(c) gene codon (# aa) (# aa) position class (# aa) AlgA TAA ND HELICc (114): 67-343 Class 1 — Helicase, ATP (277) binding, nucleic acid binding AlgB TAA ND 7 repeats of 220-485 Class 2 — Parallel beta- (265) helix (22-35): found in pectate lyases and rhamno- galacturonase A AlgC TAA ND — 295-659 Class 3 DVVVV (364) D (6) (SEQ ID NO: 70) AlgD TAG FA58C Ricin-type beta- 374-612 Class 1 Serine (131) trefoil (140) (238) stretch (24) AlgE TAG FA58C — 259-525 Class 1 TP (135) (266) stretch (39) AlgF TAA ND 9 repeats of 781-1080 Class 1 — Parallel beta- (299) helix (21-31) 1088-1461 Class 3 (373) AlgG TAA FA58C 2 copies of 361-779 Class 3 — (264), PDK1 (418) CBM-4- 9 (133) AlgH TAA CBM-4- 4 repeats of 288-553 Class 2 EGEP 9 (168) Parallel beta- (265) (47) helix (22-32) (SEQ ID NO: 69) AlgI TAG ND d1dbga (345), 217-517 Class 2 — or PDB id (276) (300) Pectin lyase- like domain AlgJ TAA FA58C — — TP (142), stretch CBM-4- (22) 9 (122) AlgK TAA ND — — — — ^(a)CBD: Carbohydrate binding domain ^(b)MMBD: Macromolecule binding domain. ^(c)For more details on repeats and their functions, see Results. ND: No determined match was identified from the genome annotation.

Genomic analysis showed that 2-40 alginases have molecular weights that vary widely from 37 to 163 kDa. Genomic annotation also showed that all of the eleven alginases of 2-40 have signal peptide, except AlgA and AlgK, which were not amenable to annotation. AlgD, AlgE, AlgG, AlgH and AlgJ have carbohydrate binding domains. Several repeats of the PbH1 domains were found in AlgB, AlgF and AlgH. AlgG contains PDK domain and could bind putative scaffold on the cell surface. 2-40 alginase protein sequences had a high level of similarity to alginases from 4 Klebsiella spp., 5 Pseudomonas spp., 1 Corynebacterium sp. and 1 Vibrio sp., suggesting (among other examples) that 2-40 is unusually adept at horizontal transfer and recombination.

The biochemistry of alginate biosynthesis has been determined in the human pathogen Pseudomonas aeruginosa and in Azotobacter vinelandii (Rehm and Valla 1997). In both organisms the immediate precursor of polymerization is GDP-mannuronic acid, and the sugar residues in this compound are polymerized into mannuronan. This polymer is then further modified by acetylation at 0-2 and/or 0-3 position(s) of some of the D-mannuronate residues. This results in the formation of alginates with different block structures and degrees of O-acetylation. In brown algae, however, alginates are not acetylated.

Based on the characterized biochemistry pathway of alginate biosynthesis and on the genomic analysis of 2-40 alginase system, a pathway for degradation and transport of alginate in 2-40 can be proposed. Since it grows on alginate as a sole carbon source, arguably 2-40 encodes an enzyme system to depolymerize, transport and metabolize alginate polymers down to monosaccharide 4-deoxy-L-erythro-5-hexoseulose uronic acid. The first stage of depolymerization would occur extracellularly and may be carried out by alginases AlgD, E, G, H and J. Alginate would be epimerized into homopolymers of mannuronic acid residues (in the case where the alginic acid contains both M and G residues). The need for more than one extracellular alginase is explained by the substrate specificities observed for alginases from various sources (Chavagnat et al., 1998, and Rehm 1998). Additionally some alginate lyase may only degrade defined oligomannuronic lengths (Rehm 1998). Other alginases may be extracellular while others may be epicellular.

In the next stage, polymannuronate (poly-M) would then be degraded into alginate-oligosaccharide and unsaturated uronic acid (AOS+UA). The AOS−UA may be transported into the periplasm via a specialized outer-membrane porin, yet to be identified. There, the unsaturated uronic acid residues would further be degraded by AlgC, B, F and I to monosaccharide 4-deoxy-L-erythro-5-hexoseulose uronic acid (MS-DEHL). This would be reduced to 2-keto-3-deoxy-D-gluconic acid (KDG) by AlgA and AlgK. KDG and then catalyzed to GDP-mannose by dehydrogenase to GDP-mannose which would go through serial reaction steps to until it is converted to fructose-6-phosphate.

In various embodiments of this invention, the alginase degrading enzymes, related proteins and systems containing thereof, of this invention, for example including one or more enzymes or alginase-binding proteins, have a number of uses. In fact, many possible uses of the alginases of the present invention are conceivable. For example Table X lists some of the uses of alginates to which the alginases of the present invention can be expected to be useful, for example in cleaning up the alginates and/or to shorten the size of the alginates.

TABLE X Type of Application Alginate Functions and Benefits FOOD Bakery Creams Protanal ® Instant gelling and thickening; heat stability; range of different textures; good mouthfeel and flavor release Dressings Protanal Ester Thickening, stabilizing, emulsifying; good mouthfeel; acid stable Fruit Juices Protanal Ester Stabilizing, emulsifying Fruit Fillings and Protanal Gelling, thickening, stabilizing; prevents syneresis; excellent heat Preparations stability; cold and hot process; wide range of different textures; available for low to high brix systems Ice Cream and Protanal Stabilizing; controlled viscosity; prevents crystal formation and Sorbet shrinkage; contributes to even and slow meltdown Low Fat Spreads Protanal Stabilizing; good mouthfeel, texture and flavor release Restructured Protanal Excellent gelling ability; heat stability; easy to form Foods Yoghurt Protanal Stabilizing; good mouthfeel, texture and flavor release SPECIALTY Beer Profoam ® Improves and maintains foam levels Petfoods Protanal Gelling of heat-resistant and retortable meat-like chunks Textile Printing Lamitex, ® Gives the desired rheology to print pastes; is inert to dyes and Scotex ® fibers; has excellent wash-out properties; is extremely pure Paper Scogin ® Enhance greaseproof properties, oil resistance, and solvent holdout; improves rheology, water-retention, runability, ink holdout, and printability Welding Protaweld ™ Lubricant stabilizer and “green strength” agent in the extrusion of high quality welding rods

The alginases of this invention have unusual versatility in degrading alginates from a wide variety of sources. Advantages of the alginases of this invention are that they can withstand high salt environments and relatively high pH. The alginases of this invention can also resist detergents.

2-40 has a very high efficiency turnover rate and the alginases produced thereby have unusual enzyme architectures.

The alginases of this invention are useful in degrading alginate polymers to produce shorter chains, for example exoalginases, that are useful as feedstock for land-based animals, as well as for fish and other marine animals.

In one embodiment, these systems can be used to degrade alginate to produce short chain peptides for use in medicine. In another embodiment, the alginase systems can be used to treat cystic fibrosis patients by administering at least one of the alginases of this invention to a patient to degrade viscous polymer produced by Psudomonas aeruginosa.

In some embodiments of this invention, alginate or algae may be used to absorb environmental pollutants and waste spills. The alginate may then be degraded by the alginate degrading systems of the present invention. Bacteria that can metabolize environmental pollutants and can degrade alginate may be used in bioreactors that degrade toxic materials. Such a bioreactor would be advantageous since there would be no need to add additional nutrients to maintain the bacteria—they would use alginate as a carbon source.

In some embodiments of this invention, alginate degrading enzyme systems can be supplied in dry form, in buffers, as pastes, paints, micelles, etc. Alginase systems can also comprise additional components such as metal ions, chelators, detergents, organic ions, inorganic ions, additional proteins such as biotin and albumin.

In some embodiments of this invention, the alginate degrading systems of this invention could be applied directly to the alginate material. For example, a system containing one, some or all of the alginases of this invention could be directly applied to algae such that the system would degrade the algae. As another example, 2-40 could be grown on algae, which would allow the 2-40 to produce the alginases of this invention in order to degrade the algae as the 2-40 grows. An advantage of using the 2-40 or systems of this invention is that the degradation of the algae can be conducted in a marine environment, for example under water.

It is one aspect of the present invention to provide a nucleotide sequence that has a homology selected from 100%, 99%, 98%, 97%, 96%, 95%, 90%, 85%, 80%, or 75% to any of the sequences of the alginases of this invention.

The present invention also covers replacement of between 1 and 20 nucleotides of any of the alginases of this invention with non-natural or non-standard nucleotides for example phosphorothioate, deoxyinosine, deoxyuridine, isocytosine, isoguanosine, ribonucleic acids including 2-O-methyl, and replacement of the phosphodiester backbone with, for example, alkyl chains, aryl groups, and protein nucleic acid (PNA).

It is another aspect of some embodiments of this invention to provide a nucleotide sequence that hybridizes to any one of the alginases of this invention under stringency condition of 1×SSC, 2×SSC, 3×SSC1, 4×SSC, 5×SSC, 6×SSC, 7×SSC, 8×SSC, 9×SSC, or 10×SSC.

The scope of this invention covers natural and non-natural alleles of any one of the sequences of the alginases of this invention. In some embodiments of this invention, alleles of any one of any one of the sequences of the alginases can comprise replacement of one, two, three, four, or five naturally occurring amino acids with similarly charged, shaped, sized, or situated amino acids (conservative substitutions). The present invention also covers non-natural or non-standard amino acids for example selenocysteine, pyrrolysine, 4-hydroxyproline, 5-hydroxylysine, phosphoserine, phosphotyrosine, and the d-isomers of the 20 standard amino acids.

It is to be understood that while the invention has been described above using specific embodiments, the description and examples are intended to illustrate the structural and functional principles of the present invention and are not intended to limit the scope of the invention. On the contrary, the present invention is intended to encompass all modifications, alterations, and substitutions within the spirit and scope of the appended claims.

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1. Isolated AlgF comprising SEQ ID NO:
 44. 2. A kit comprising a sealed containing AlgF comprising SEQ ID NO:44. 